Proteinase k free nucleic acid extraction buffer system

ABSTRACT

A GRD buffer system, which is free of proteinase K, for extracting nucleic acid is provided. The GRD buffer system comprises a GRD lysis buffer (GRD-LB), a GRD wash buffer (GRD-WB), and a GRD elution buffer (GRD-EB). Also provided is a method of extracting nucleic acid with the above GRD buffer system.

CROSS-REFERENCE TO RELATED APPLICATION

This application claims the benefit of U.S. Provisional Application No. 63/188,318, filed May 13, 2021, and is a divisional of U.S. Nonprovisional application Ser. No. 17/560,573, filed Dec. 23, 2021; the contents of which are incorporated by reference herein in their entirety.

SEQUENCE LISTING

The instant application contains a Sequence Listing which has been submitted electronically in ASCII format and is hereby incorporated by reference in its entirety. Said ASCII copy, created on May 11, 2022, is named REDI-02-US_SL.txt and is 16,717 bytes in size.

BACKGROUND OF THE INVENTION (1) Field of the Invention

The present invention relates to multiplex detection of nucleic acid sequences. More particularly, a composition and method for detecting nucleic acids in samples, e.g., clinical samples is provided. The composition and method provide highly sensitive assays with a very low background.

(2) Description of the Related Art

From the avian flu to severe acute respiratory syndrome (SARS) and other coronaviruses, such as the SARS COV-2 virus that causes the COVID-19 disease, respiratory viruses are currently the cause of great concern worldwide. Approximately 500 million non-influenza related viral respiratory tract infections (VRTI) episodes occur per year in the United States. These episodes have had an enormous cost in terms of lost lives, destroyed livelihoods, and negative financial impact throughout the world. Some respiratory virus illnesses cause a heavy burden in terms of morbidity and mortality, primarily among infants and the elderly. Moreover, it is often difficult to distinguish between the different possible causes of respiratory infections. Many viruses have similar symptomology and their precise diagnosis often requires high-complexity laboratory testing. Because of cost and technical limitations, such testing is sporadically performed and only for a limited number of viruses.

For example, traditional detection of respiratory viruses involves viral propagation in cell culture with or without direct immunoassays. Though very specific, this method has many disadvantages, as it often lacks sensitivity, is burdensome, requires skilled personnel, and takes between five and ten days before obtaining results. To more efficiently detect respiratory viruses, immunoassays have been developed that measure the titre of a virus using the reaction of an antibody to its antigen (e.g., various immunoassays are commercially available for influenza A detection). While relatively inexpensive and rapid, immunoassays are typically limited to the detection of a single virus species, and have reduced sensitivity and specificity. In addition, the development of such tests is impractical for some viruses having many subtypes including for example, enteroviruses.

In response to these deficiencies, certain tests have been developed that use multiplex polymerase chain reaction (PCR) to detect many viruses in one assay. Examples for such PCR-based tests are described in U.S. Pat. No. 6,015,664 to Henrickson, and U.S. Pat. No. 6,881,835 to Bai et al. Both Henrickson and Bai utilize primers in a PCR process to amplify viral sequences if present in the sample. The amplified sequences are then hybridized to a solid support. One problem with these methods is the many required washing steps that can result in loss of signal and/or additional noise in the results, as well as increased time and cost for handling and detection. Furthermore, at least some of the detection methods can be cumbersome and have a relatively low sensitivity.

Although many kits and methods for respiratory virus detection are known in the art, all or almost all of them suffer from one or more disadvantages. Thus, there is still a need to provide kits and methods for detecting a plurality of respiratory viruses using a multiplex assay. As disclosed in US Patent Application Publication 2011/0046001, there are samples, kits, and methods that detect at least two respiratory viruses using a multiplexed diagnostic assay. According to US20110046001, the respiratory virus can be any DNA or RNA virus affecting the respiratory system including for example, an adenovirus, a coronavirus, an enterovirus, a rhinovirus, an influenza virus, a human metapneumovirus (HMPV), a human respiratory syncytial virus (HRSV), a human parainfluenza virus (HPIV), as well as all sero- and genotypes and combinations thereof. The limitations of the current state of the art assay process is exemplified by the ThermoFisher TaqPath® COVID multiplex assay process. In the current process, MS2 Phage is used as a control: MS2 phage must be kept at negative twenty degrees Celsius (−20° C.) for working stocks. MS2 phage is exogenous (added to each sample) and thus, is incapable of determining sample integrity. The stability and reproducibility of the MS2 phage control is poor. Additionally, in the current process, RNA control is used for PCR. Such RNA controls require manipulation before use (i.e. dilutions, which increase labor cost and subsequently decreases stability based on technical user error). RNA controls also increase workflow as illustrated and described in FIG. 1. Accordingly, a better control with improved accuracy, reduced labor, less paths for introduction of errors, and stability of the control at temperatures that are above the freezing point of water and can be maintained by a standard refrigeration cycle without requiring frozen temperatures.

Additionally, as illustrated in FIG. 2, background noise of the currently known assay increases variability in the analysis. It would be beneficial to reduce the background noise to reduce variability in the analysis and increase the sensitivity to the virus detection.

It is also important to recognize that some of the same symptoms of COVID-19 caused by the SARS-CoV-2 virus are similar to the symptoms of influenza viruses. Accordingly, a test that is merely capable of detecting only the presence of SARS-CoV-2 and is not capable of simultaneously determining the presence of influenza viruses is less beneficial to caregivers and their patients than a multiplex assay that allows for the simultaneous detection of influenza A, influenza B, and SARS-CoV-2.

It will also be appreciated that a test could have absolutely perfect accuracy and could be a foolproof process with absolutely no error path in the process, but if accessibility of the test is limited to hospitals and specialty clinics, the value of the perfect accuracy and foolproof process are greatly diminished because testing must be accessible to a large percentage of the population for the testing to be effective. Accordingly, in addition to improved accuracy of tests, the accessibility to tests and the convenience of patients in getting tested is also an important factor for an improved multiplex assay.

Other multiplex PCR assays include those described in US Patent Application Publication 20070207453.

BRIEF SUMMARY OF THE INVENTION

The present invention is to provide a GRD buffer system, free of proteinase K, for extracting nucleic acid, in procedures using polymerase chain reaction (PCR) to detect more than one target nucleic acid sequence, e.g., nucleic acid from more than one virus in a mammalian tissue or fluid sample, certain methodologies and reagents provide results with surprisingly low background with higher sensitivity than achieved in the prior art.

Thus, in some embodiments, a composition, free of proteinase K, for extracting nucleic acid for detecting more than one target nucleic acid sequence in a nucleic acid sample by polymerase chain reaction (PCR) is provided. In these embodiments, the composition comprises

a GRD lysis buffer (GRD-LB), wherein the GRD-LB comprises a first buffer and a first chaotropic agent;

a GRD wash buffer (GRD-WB), wherein the GRD-WB comprises a second buffer, a second chaotropic agent, and an alcohol;

a GRD elution buffer (GRD-EB), wherein the GRD-EB comprises a third buffer; and

the GRD buffer system is free of proteinase K.

Also provided is a method of extracting nucleic acid with the GRD buffer system. The method comprises

providing a sample; and

extracting nucleic acid with the GRD buffer system.

BRIEF DESCRIPTION OF THE SEVERAL VIEWS OF THE DRAWINGS

FIG. 1 is a flow chart showing the workflow of a prior art multiplex assay.

FIG. 2 is a graph showing representative results from a prior art multiplex assay.

FIG. 3 is an annotated construct map for the pMK-FluV19 control plasmid.

FIG. 4 is a graph showing representative results using a composition and method of the present invention. Those methods show surprisingly low background levels as well as greater analytical sensitivity and accuracy than prior art methods.

FIGS. 5A, 5B, 5C and 5D are graphs showing Reditus extraction reagents (GRD; alternatively abbreviated as ReX in U.S. Provisional Application No. 63/188,318, filed May 13, 2021 and U.S. Nonprovisional application Ser. No. 17/560,573, filed Dec. 23, 2021) for the invention assay are equivalent to those in MagMax™ Viral and Pathogen Nucleic Acid Isolation Kits. A single high-positive (low Cq) SARS-CoV-2 positive clinical specimen was diluted in 0.5 log increments using a clinical-negative specimen as diluent. Each dilution was extracted in triplicated using either Reditus extraction reagents (GRD) or MagMax reagents. Extracted nucleic acid was amplified using Thermo TaqPath COVID-19 Combo Kit RT-PCR reagents and analyzed using Applied Biosystems Design & Analysis Software. SARS-CoV-2 gene targets (FIG. 5A. N-gene, FIG. 5B. S-gene, FIG. 5C. ORF lab) and the MS2 phage (FIG. 5D) were analyzed and graphed using the mean±sem of each replicate dilution.

FIGS. 6A, 6B, 6C, 6D, 6E, 6F, 6G and 6H are graphs showing that the Reditus extraction reagents (GRD) demonstrate less variability in extraction than MagMax™ Viral and Pathogen Nucleic Acid Isolation Kits. A total of n=5 SARS-CoV-2 positive specimens were identified and extracted in triplicate over 5 Days (7=25 data points) using either Reditus extraction reagents (GRD) or MagMax reagents. Extracted nucleic acid was amplified using Thermo TaqPath COVID-19 Combo Kit RT-PCR reagents and analyzed using Applied Biosystems Design & Analysis Software. Each viral gene target and extraction target (MS2 phage) was analyzed for the mean±sem of each triplicate per day (n=25 averaged data points) and is presented in FIGS. 6A, 6C, 6E and 6G. The variance in extraction was assessed in each gene target detection FIGS. 6B, 6D, 6F, and 6H) over 5-Days (1=75) and represents the statistical “true value (V_(T))” for each sample. The experimental bias (Vs) was calculated for each extraction process as defined by

$V_{B} = {\frac{\sum\left\lbrack {{V_{E} - V_{T\; 1}},{V_{E} - V_{T\; 2}},{V_{E} - {V_{T\; 3}\mspace{14mu}\ldots\mspace{14mu} V_{E}} - V_{T\; 25}}} \right\rbrack}{DF}.}$

FIGS. 7A and 7B are graphs showing effectiveness of total human RNA control as a non-viral extraction control (NVC). Human total RNA control (50 ng/μl) was purchased from Applied Biosystems (Cat #4307281, Foster City, Calif.). Total control RNA was diluted to a starting concentration of 1.0 ng/μl in 10 mM Tris and serial diluted in a final volume of 1 ml at 0.5 log increments in Tris (pH 8.0) from 1.0 ng/μl to 0.0316 ng/μl. A total of 200 μl of each dilution was extracted in triplicate using GRD reagents on the KingFisher extraction platform and analyzed by RT-PCR on a QuantStudio 12K Flex real-time instrument using 5 μl of elution in a total reaction volume of 20 μl. A predefined amplification range for RNase P was established at 28±2 cycles (grey zone in FIGS. 7A and 7B) and concentrations of RNase P which fell within range following 200 μl extraction are depicted in FIG. 7A. Stability of the NVC was established over time (FIG. 7B) when stored at 2-8° C. from 1 to 24 hours. The 0-hour represents the time at which a fresh NVC was prepared and the total change of n=3 replicates were tested and compared against the 0-hour timepoint. All graphed data in FIGS. 7A and 7B represent the mean±sem of n=3 replicates.

FIGS. 8A, 8B, 8C and 8D are graphs showing the Reditus FluV19 assay is equivalent to the EUA-CDC FLuSC2 assay. Linearized pMK-FluV19 plasmid were diluted in 0.5 log increments using 10 mM Tris (pH 8.0) as the diluent. 5 μl of total input was analyzed by PCR using either the FluV19 PCR reaction mix depicted in Table 4 or in accordance with the EUA CDC-FLuSC2 method. Each dilution was tested in triplicate and the mean±sem of each dilution is presented in for each gene target (FIG. 8A, Influenza A; FIG. 8B, Influenza B; FIG. 8C, SARS-CoV-2, and FIG. 8D, RNase P).

FIGS. 9A, 9B and 9C are graphs showing results of single-positive clinical samples tested by GRD FluV19, CDC-FLuSC2, and Thermo Fisher TaqMan COVID-19 FluA/B Multiplex RT-PCR Assays. Single-positive clinical specimens were extracted using either Reditus extraction reagents (GRD) or MagMax reagents. Nucleic acid extracted from specimens using GRD reagents were amplified using the FluV19 assay reaction mixture specified in Table 4. Nucleic acid from specimens extracted using MagMax reagents were amplified using either the CDC-FLuSC2 assay or Thermo TaqPath COVID-19 FluA/B RT-PCR reagents according to each manufacturer's requirements. FIG. 9A: Analysis of clinical sample amplification for Influenza A using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). FIG. 9B: Analysis of clinical sample amplification for Influenza B using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). FIG. 9C: Analysis of clinical sample amplification for SARS-CoV-2 using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). Each data point represents a single extraction and analysis to represent testing and analysis of clinical samples.

FIGS. 10A and 10B are graphs showing results of influenza A and influenza B double-positive clinical samples tested by GRD FluV19, CDC-FLuSC2, and Thermo Fisher TaqMan COVID-19 FluA/B Multiplex RT-PCR assays. Influenza A and influenza B clinical specimens were combined to generate specimens representing dual infections at high (H) and low (L) concentrations. Each specimen was extracted using either Reditus extraction reagents (GRD) or MagMax reagents. Nucleic acid extracted from specimens using GRD reagents were amplified using the FluV19 assay reaction mixture specified in Table 4. Nucleic acid from specimens extracted using MagMax reagents were amplified using either the CDC-FLuSC2 assay or Thermo TaqPath COVID-19 FluA/B RT-PCR reagents according to each manufacturer's requirements. FIG. 10A: Analysis of clinical sample amplification for influenza A using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). FIG. 10B: Analysis of clinical sample amplification for influenza B using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). Each data point represents a single extraction and analysis to represent testing and analysis of clinical samples.

FIGS. 11A and 11B are graphs showing results of influenza A and SARS-CoV-2 double-positive clinical samples tested by GRD FluV19, CDC-FLuSC2, and Thermo Fisher TaqMan COVID-19 FluA/B Multiplex RT-PCR Assays. Influenza A and SARS-CoV-2 clinical specimens were combined to generate specimens representing dual infections at high (H) and low (L) concentrations. Each specimen was extracted using either Reditus extraction reagents (GRD) or MagMax reagents. Nucleic acid extracted from specimens using GRD reagents were amplified using the FluV19 assay reaction mixture specified in Table 4. Nucleic acid from specimens extracted using MagMax reagents were amplified using either the CDC-FLuSC2 assay or Thermo TaqPath COVID-19 FluA/B RT-PCR reagents according to each manufacturer's requirements. FIG. 11A: Analysis of clinical sample amplification for influenza A using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). FIG. 11B: Analysis of clinical sample amplification for SARS-CoV-2 using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). Each data point represents a single extraction and analysis to represent testing and analysis of clinical samples.

FIGS. 12A and 12B are graphs showing results of influenza B and SARS-CoV-2 double-positive clinical samples tested by GRD FluV19, CDC-FLuSC2, and Thermo Fisher TaqMan COVID-19 FluA/B Multiplex RT-PCR Assays. Influenza B and SARS-CoV-2 clinical specimens were combined to generate specimens representing dual infections at high (H) and low (L) concentrations. Each specimen was extracted using either Reditus extraction reagents (GRD) or MagMax reagents. Nucleic acid extracted from specimens using GRD reagents were amplified using the FluV19 assay reaction mixture specified in Table 4. Nucleic acid from specimens extracted using MagMax reagents were amplified using either the CDC-FLuSC2 assay or Thermo TaqPath COVID-19 FluA/B RT-PCR reagents according to each manufacturer's requirements. FIG. 12A: Analysis of clinical sample amplification for influenza B using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). FIG. 12B: Analysis of clinical sample amplification for SARS-CoV-2 using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). Each data point represents a single extraction and analysis to represent testing and analysis of clinical samples.

FIGS. 13A, 13B and 13C are graphs showing results of influenza A, influenza B, and SARS-CoV-2 Combined-Positive Clinical Samples Tested by GRD FluV19, CDC-FLuSC2, and Thermo Fisher TaqMan COVID-19 FluA/B Multiplex RT-PCR Assays. Influenza A, influenza B and SARS-CoV-2 clinical specimens were combined to generate specimens representing unlikely but possible triple infections at high (H) and low (L) concentrations. Each specimen was extracted using either Reditus extraction reagents (GRD) or MagMax reagents. Nucleic acid extracted from specimens using GRD reagents were amplified using the FluV19 assay reaction mixture specified in Table 4. Nucleic acid from specimens extracted using MagMax reagents were amplified using either the CDC-FLuSC2 assay or Thermo TaqPath COVID-19 FluA/B RT-PCR reagents according to each manufacturer's requirements. FIG. 13A: Analysis of clinical sample amplification for influenza A using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). FIG. 13B: Analysis of clinical sample amplification for influenza B using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). FIG. 13C. Analysis of clinical sample amplification for SARS-CoV-2 using FluV19 (closed black bar), FLuSC2 (closed grey bar), or COVID-19 FluA/B (open white bar). Each data point represents a single extraction and analysis to represent testing and analysis of clinical samples.

FIG. 14 is an annotated map of pFRV19.

DETAILED DESCRIPTION OF THE INVENTION

The present invention is to provide a GRD buffer system, free of proteinase K, for extracting nucleic acid, in procedures using polymerase chain reaction (PCR) to detect more than one target nucleic acid sequence, e.g., nucleic acid from more than one virus in a mammalian tissue or fluid sample, certain methodologies and reagents provide results with surprisingly low background with higher sensitivity than achieved in the prior art. See Example.

Thus, in some embodiments, a composition, free of proteinase K, for extracting nucleic acid for detecting more than one target nucleic acid sequence in a nucleic acid sample by polymerase chain reaction (PCR) is provided. In these embodiments, the composition comprises a GRD lysis buffer (GRD-LB), wherein the GRD-LB comprises a first buffer and a first chaotropic agent;

a GRD wash buffer (GRD-WB), wherein the GRD-WB comprises a second buffer, a second chaotropic agent, and an alcohol;

a GRD elution buffer (GRD-EB), wherein the GRD-EB comprises a third buffer; and

the GRD buffer system is free of proteinase K.

In some embodiments, the GRD-LB further comprises a first chelating agent, a first detergent, a first denaturant, and a dye.

In some embodiments, the GRD-WB further comprises a second chelating agent.

In some embodiments, the GRD-EB further comprises a third chelating agent.

A buffer in a biological system is to maintain intracellular and extracellular pH within a very narrow range and resist changes in pH in the presence of internal and external influences. The pH in a biological system controls the solubility, biological functions, and the chemical reactivity of biomaterials. Nonlimiting examples of the buffer comprises IVIES, Bis-Tris Propane, TES, HEPES, DIPSO, MOBS, TAPSO, Tris, Trizma, HEPPSO, POPSO, TEA, EPPS, Tricine, Gly-Gly, Bicine, HEPBS, TAPS, AMPD, TABS, AMPSO, CHES, CAPSO, AMP, CAPS, and CABS.

In some embodiments, the buffer comprises Bis-Tris Propane, TES, HEPES, DIPSO, MOBS, TAPSO, Tris, Trizma, HEPPSO, POPSO, TEA, EPPS, Tricine, Gly-Gly, Bicine, HEPBS, TAPS, and AMPD.

In some embodiments, the first buffer, the second buffer, and the third buffer are independently selected from Bis-Tris Propane, TES, HEPES, DIPSO, MOBS, TAPSO, Tris, Trizma, HEPPSO, POPSO, TEA, EPPS, Tricine, Gly-Gly, Bicine, HEPBS, TAPS, and AMPD.

In some embodiments, the first buffer, the second buffer, and the third buffer are Tris (pH 8.0, Cf=10-100 mM).

A chaotropic agent disrupts the hydrogen bonding network in water solution, destabilizing the native state of macromolecules (e.g. proteins, nucleic acids) in the solution. The chaotropic agent denatures nucleic acids associated proteins, therefore weakening the hydrophobic interaction between nucleic acids associated proteins and nucleic acids. The chaotropic agent dissociates nucleic acids from nucleic acids associated proteins and allows nucleic acids to be extracted in subsequent purification step. Nonlimiting examples of the chaotropic agent comprises guanidinium thiocyanate, guanidine, urea, and thiourea.

In some embodiments, the chaotropic agent comprises guanidinium thiocyanate (Cf=0.5 M-10 M).

In some embodiments, the first chaotropic agent comprises guanidinium thiocyanate (Cf=4 M) and the second chaotropic agent comprises guanidinium thiocyanate (Cf=1.82 M).

A chelating agent is a chemical compound that reacts with metal ions to form stable, water-soluble metal complexes. The presence of the chelating agent in a biological sample protects nucleic acids from enzymatic degradation by removing the metal ions. The chelating agent also reduces interaction between proteins and nucleic acids, therefore enhancing the nucleic acids extraction efficiency in a biological sample. Nonlimiting examples of the chelating agent comprises EDTA, EGTA, HEDTA, NTA, and TEA.

In some embodiments, the chelating agent comprises EDTA ((pH 8.0, Cf=1 mM-500 mM).

In some embodiments, the chelating agent comprises EDTA (pH 8.0, Cf=7.5 mM-25 mM).

A detergent is a surfactant with an amphiphilic structure, where each molecule has a hydrophilic (polar) head and a long hydrophobic (non-polar) tail. The dual nature of the detergent facilitates the mixture of hydrophobic compounds with water, e.g. in a biological sample.

Nonlimiting examples of the detergent comprises Triton X-100, TWEEN-20, NP-40, and Brij-35.

In some embodiments, the detergent comprises Triton X-100 (1%-10% v/v).

In some embodiments, the detergent comprises Triton X-100 (3% v/v).

A denaturant is a molecular that causes other proteins or nucleic acids to lose their quaternary structure, tertiary structure, and secondary structure which is present in their native state. The denaturant dissociates nucleic acids from nucleic acids associated proteins and allows nucleic acids to be extracted in subsequent purification step. Nonlimiting examples of the denaturant comprises formamide, guanidine, sodium salicylate, dimethyl sulfoxide (DMSO), propylene glycol, and urea.

In some embodiments, the denaturant comprises urea (Cf=1 mM-10 M).

In some embodiments, the denaturant comprises urea (Cf=10 mM).

Alcohol precipitation is a technique for concentrating and de-salting nucleic acid (DNA or RNA) preparations in an aqueous solution. Nonlimiting examples of the alcohol comprises methanol, ethanol, and isopropanol.

In some embodiments, the alcohol comprises ethanol (Cf=70% v/v).

Bromophenol blue, xylene cyanol, and orange G are organic dyes that are used to mark the biological sample without interfering with the nucleic acids.

In some embodiments, the dye comprises bromophenol blue (Cf=0.01% v/v).

Also provided is a method of extracting nucleic acid with the GRD buffer system. The method comprises

providing a sample; and

extracting nucleic acid with the GRD buffer system.

In some embodiments, the sample is from a nasal swab, a nasopharyngeal swab, or a throat swab.

In some embodiments, the sample contains a respiratory virus, wherein the respiratory virus is influenza A, influenza B, SARS-CoV-2, respiratory syncytial virus subtype A, respiratory syncytial virus subtype B, or any combination thereof is from a nasal swab, a nasopharyngeal swab, or a throat swab. See Examples below.

The present invention is based in part on the discovery that, in procedures using polymerase chain reaction (PCR) to detect more than one target nucleic acid sequence, e.g., nucleic acid from more than one virus in a mammalian tissue or fluid sample, certain methodologies and reagents provide results with surprisingly low background with less variability, while utilizing reagents that are simplified compared to prior art assays. See Example.

Thus, in some embodiments, a composition for detecting more than one target nucleic acid sequence in a nucleic acid sample by polymerase chain reaction (PCR) is provided. In these embodiments, the composition comprises

a plasmid comprising (a) a transcribable target sequence of each of the more than one virus, and (b) a sequence encoding a portion of a human housekeeping gene;

a passive reference dye; and

a set of two DNA primers and a DNA probe for each of the more than one virus and the portion of the RNase P, wherein the probe comprises a dye.

These compositions can be utilized to detect any useful target nucleic acid sequence, including but not limited to sequences in environmental samples (e.g., wastewater, soil, river samples, ocean samples, etc.), or samples from living, inactive or deceased organisms such as archaea, prokaryotes or eukaryotes, e.g., protists, invertebrates, or vertebrates such as mammals, including humans. In some embodiments, the nucleic acid sample is from a mammalian tissue or fluid sample such as a biopsy, urine, feces, blood, mucus, etc. In particular embodiments, the mammalian tissue or fluid sample is a human nasal swab.

Nonlimiting examples of the target nucleic acid sequences are sequences associated with a disease, for example cancer or a disease of genetic etiology, e.g., genetic abnormalities in a fetus, child or adult. In some embodiments, the target nucleic acid sequence is from a disease organism such as a bacteria, fungus or protist.

In various embodiments, at least one of the more than one target nucleic acid sequence is from a virus. The virus in these embodiments can be any virus now known or later discovered. Non-limiting examples include the herpes virus (e.g., human cytomegalomous virus (HCMV), herpes simplex virus 1 (HSV-1), herpes simplex virus 2 (HSV-2), varicella zoster virus (VZV), Epstein-Barr virus), influenza A virus, influenza B virus, or a picornavirus such as Coxsackievirus B3 (CVB3). Other viruses include, but are not limited to, hepatitis B virus, HIV, poxvirus, hepadavirus, a retrovirus, and RNA viruses such as flavivirus, togavirus, coronavirus, Hepatitis D virus, orthomyxovirus, paramyxovirus, rhabdovirus, bunyavirus, filo virus, adenovirus, human herpesvirus, type 8, human papillomavirus, BK virus, JC virus, smallpox, hepatitis B virus, human bocavirus, parvovirus B19, human astrovirus, Norwalk virus, coxsackievirus, hepatitis A virus, poliovirus, rhinovirus, severe acute respiratory syndrome (SARS) virus, SARS-CoV-2 virus, hepatitis C virus, yellow fever virus, dengue virus, West Nile virus, Rubella virus, Hepatitis E virus, and Human immunodeficiency virus (HIV). In some cases, the virus is an enveloped virus. Examples include, but are not limited to, viruses that are members of the hepadnavirus family, herpesvirus family, iridovirus family, poxvirus family, flavivirus family, togavirus family, retrovirus family, coronavirus family, filovirus family, rhabdovirus family, bunyavirus family, orthomyxovirus family, paramyxovirus family, and arenavirus family. Other examples include, but are not limited to, hepadnavirus hepatitis B virus (HBV), woodchuck hepatitis virus, ground squirrel (Hepadnaviridae) hepatitis virus, duck hepatitis B virus, heron hepatitis B virus, herpesvirus herpes simplex virus (HSV) types 1 and 2, varicella-zoster virus, cytomegalovirus (CMV), human cytomegalovirus (HCMV), mouse cytomegalovirus (MCMV), guinea pig cytomegalovirus (GPCMV), Epstein-Barr virus (EBV), human herpes virus 6 (HHV variants A and B), human herpes virus 7 (HHV-7), human herpes virus 8 (HHV-8), Kaposi's sarcoma-associated herpes virus (KSHV), B virus Poxvirus vaccinia virus, variola virus, smallpox virus, monkeypox virus, cowpox virus, camelpox virus, ectromelia virus, mousepox virus, rabbitpox viruses, raccoonpox viruses, molluscum contagiosum virus, orf virus, milker's nodes virus, bovin papullar stomatitis virus, sheeppox virus, goatpox virus, lumpy skin disease virus, fowlpox virus, canarypox virus, pigeonpox virus, sparrowpox virus, myxoma virus, hare fibroma virus, rabbit fibroma virus, squirrel fibroma viruses, swinepox virus, tanapox virus, yabapox virus, flavivirus dengue virus, hepatitis C virus (HCV), GB hepatitis viruses (GBV-A, GBV-B and GBV-C), West Nile virus, yellow fever virus, St. Louis encephalitis virus, Japanese encephalitis virus, Powassan virus, tick-borne encephalitis virus, Kyasanur Forest disease virus, Togavirus, Venezuelan equine encephalitis (VEE) virus, chikungunya virus, Ross River virus, Mayaro virus, Sindbis virus, rubella virus, retrovirus human immunodeficiency virus (HIV) types 1 and 2, human T cell leukemia virus (HTLV) types 1, 2, and 5, mouse mammary tumor virus (MMTV), Rous sarcoma virus (RSV), lentiviruses, Filovirus Ebola virus, Marburg virus, metapneumoviruses (MPV) such as human metapneumovirus (HMPV), rhabdovirus rabies virus, vesicular stomatitis virus, Bunyavirus, Crimean-Congo hemorrhagic fever virus, Rift Valley fever virus, La Crosse virus, Hantaan virus, Orthomyxovirus, influenza virus (types A, B, and C), Paramyxovirus, parainfluenza virus (PIV types 1, 2 and 3), respiratory syncytial virus (subtypes A and B), measles virus, mumps virus, Arenavirus, lymphocytic choriomeningitis virus, Junin virus, Machupo virus, Guanarito virus, Lassa virus, Ampari virus, Flexal virus, Ippy virus, Mobala virus, Mopeia virus, Latino virus, Parana virus, Pichinde virus, Punta toro virus (PTV), Tacaribe virus and Tamiami virus. In some embodiments, the virus is influenza A virus, e.g., strain H1N1.

In various embodiments, at least one of the more than one virus is an RNA virus, for example a respiratory virus. Specific examples include influenza A, influenza B, SARS-CoV-2, respiratory syncytial virus subtype A and respiratory syncytial virus subtype B.

In some embodiments, the more than one target nucleic acid sequence is RNA from at least two, three, four or five viruses selected from the group consisting of influenza A, influenza B, SARS-CoV-2, respiratory syncytial virus subtype A and respiratory syncytial virus subtype B. In certain embodiments, the more than one target nucleic acid sequence is RNA virus is influenza A, influenza B, and/or SARS-CoV-2. In other embodiments, the more than one target nucleic acid sequence is RNA virus is influenza A, influenza B, SARS-CoV-2, respiratory syncytial virus subtype A and/or respiratory syncytial virus subtype B.

As discussed in the Example, the inclusion of a passive reference dye for data normalization. Any appropriate dye, e.g., any fluorescent dye, can be utilized, provided the dye does not interfere with other dyes used in the assay, for example the dyes on the probes. The determination of a particular dye for any assay can be made by the skilled artisan without undue experimentation. Nonlimiting examples of useful dyes include FAM, TET, JOE, VIC, HEX, Cy3, NED, TAMRA, Cy3.5, ROX, Texas Red, Cy5, and Cy5.5. In specific embodiments, the passive reference dye is ROX (see Example).

The housekeeping gene is amplified as an endogenous control for extraction and sample integrity, to detect specimens compromised by, for instance, improper storage during transport or insufficient sampling. See Example. Any housekeeping gene in the sampled organism can be used in these embodiments. Nonlimiting examples of housekeeping genes that could be utilized in these compositions include RNase P, ACTB, B2M, GAPD, GUSB, HPRT1, PGK, PP1A, RPL13A, TBP, ubiquitin and TFRC. In some embodiments, more than one housekeeping gene is amplified. In specific embodiments, the housekeeping gene is RNase P. See Example.

Where the target nucleic acid sequence is an RNA, e.g., from an RNA virus or from an expressed gene in an organism, the invention compositions should provide for reverse transcription of the target RNA to DNA for PCR. Thus, in some embodiments, the composition further comprises reverse transcriptase.

In further embodiments where a target nucleic acid sequence is RNA, the composition further comprises total RNA, e.g., from a species from where the nucleic acid sample was derived. Where the sample was derived from a human, the total RNA is total human RNA. The use of defined concentrations of total RNA can be as a non-viral control that is extracted alongside clinical specimens to assess extraction efficiency and reverse transcriptase activity of the reverse transcriptase enzyme.

The selection of primers and probes for the each target nucleic acid sequence can be made by the skilled artisan without undue experimentation. In some embodiments, the primers and probes comprise DNA sequences comprising 1, 2, 3, 4, 5, 6, 7, 8, 9, 10, 11, 12, 13, 14, 15, 16, 17, 18, 19, or all 20 of SEQ ID NOs:1-20.

Similarly, the selection of the portion of each of the more than one target nucleic acid sequence can be made by the skilled artisan without undue experimentation. In some embodiments, wherein the plasmid comprises 1, 2, 3, 4, 5 or all 6 of SEQ ID NO:21-26. In specific embodiments the plasmid comprises a sequence at least 80%, 85%, 90%, 98%, 99%, or 100% identical to SEQ ID NO:28 or 29.

The present invention also provides a kit comprising the composition of claim 1 with additional reagents for performing PCR using the plasmid, dye, primers and probes to detect the more than one target nucleic acid sequence. When supplied as a kit, the different components of the composition can be packaged in separate containers and admixed immediately before use. Such packaging of the components separately can, if desired, be presented in a pack containing the composition. The pack may, for example, comprise metal or plastic foil such as a blister pack. Such packaging of the components separately can also, in certain instances, permit long-term storage without losing activity of the components.

Any reagents required or optional to detect the target nucleic acid sequences can be included in the kit, including, for example, enzymes, nucleotides, buffers, sterile water, etc.

In certain embodiments, kits can be supplied with instructional materials. Instructions may be printed on paper or other substrate, and/or may be supplied as an electronic-readable medium, such as a thumb drive, CD-ROM, DVD-ROM, video, audio, and the like. Detailed instructions may not be physically associated with the kit; instead, a user may be directed to an Internet web site specified by the manufacturer or distributor of the kit.

Also provided is a method for detecting more than one target nucleic acid sequence in a nucleic acid sample by polymerase chain reaction (PCR). The method comprises obtaining the above-identified kit;

performing PCR on the sample and the plasmid;

analyzing results from the PCR; and

determining whether at least one of the more than one target nucleic acid sequence is in the sample.

As discussed above, the target nucleic acid sequence can be from any organism or virus. In some embodiments, the more than one target sequence is each an RNA virus. In other embodiments, the more than one target sequence is each a respiratory virus, e.g., influenza A, influenza B, SARS-CoV-2, respiratory syncytial virus subtype A and/or respiratory syncytial virus subtype B.

Also as discussed above, the sample can be from any source. In some embodiments, the sample is from a nasal swab.

Other aspects of these methods are discussed in the Examples.

The compositions and methods provided herein provide multiple advantages over current assays. For example, the assays described in the Examples provide simplified reagents for quality control.

In the currently approved method, an RNA control is used to monitor both PCR and extraction efficiency. Preparation of the control RNA involves a complicated process that is highly susceptible to error and that needs to be repeated alongside each batch of clinical specimens.

For quality control, the invention assay, exemplified in the Examples, utilizes a plasmid DNA construct and total human RNA. The plasmid contains the same influenza and SARS-2-CoV genomic sequences used for detection during PCR. The plasmid can be supplied as a stable working stock that without any manipulation serves as a positive control for PCR efficiency and master mix composition. As a control for RNA extraction and cDNA synthesis, the assay uses total human RNA containing RNase P transcript. Since the RNase P target sequence is located in an exon and does not contain intron sequence, the use of human RNA provides a more accurate indication of RNA integrity and extraction than the DNA-containing human specimen control (HSC) used in the current CDC assay or the MS2 phage exogenous control employed by the ThermoFisher COVID19 Control protocol.

The use of separate controls for PCR efficiency and RNA extraction is also more informative for troubleshooting in the event of a quality control failure and since they require no manipulation before use, eliminates the possibility of technical errors made during their preparation. Table 1 below summarizes the workflow to troubleshoot quality control failures. The present assay demonstrates where the quality control failure could occur during the testing process.

TABLE 1 CONTROL RESULT DIAGNOSIS Thermo COVID19 Control Pass None and CDC: FluSC2 PC Fail Error made in PTC preparation, poor extraction efficiency, or problem with PCR component Reditus: Plasmid/RNA Pass/Pass None Pass/Fail Poor extraction efficiency or problem with reverse transcription Fail/Pass Problem with PCR primers/probes Fail/Fail Problem with PCR master mix

According to the innovative multiplex assay as particularly described above, as exemplified in the Examples, it will be appreciated that the present invention provides multiple benefits over the current state of the art process. Features and benefits of the present invention are juxtaposed with the state of the art in Table 2 below.

TABLE 2 ThermoFisher TaqPath ® COVID Multiplex Assay Process Multiplex Assay Innovation by Reditus MS2 Phase as a control: MS2 phage must be RNase P as the control-which produces better stored at negative twenty degrees Celsius reporting accuracy. This takes the risk of false (−20° C.). MS2 phage is exogenous negatives due to the ability to detect human (added to each sample) and thus, is incapable cells within the sample. This also helps of determining sample integrity. The stability determine viability and quality of the and reproducibility of the MS2 phage control specimen. is poor. RNA control for PCR: RNA controls require Plasmid based PCR control. This is stable at manipulation before use (i.e. dilutions, which positive four degrees Celsius (+4° C.). There is increase labor cost and subsequently decreases no manipulation or dilution needed before use. stability based on technical user error). RNA This decreases user error, increases sensitivity, controls also increase workflow as illustrated and decreases labor costs. and described in FIG. 1. No passive reference dye: Lack of a passive A commercial PCR mix containing ROX reference dye in PCR reactions leads to passive reference dye is used to reduce increased background noise of the assay background noise and increase the sensitivity which increases variability in analysis in the SARS CoV2, Influenza A, and Influenza (illustrated in FIG. 2). B detection. This is illustrated in FIG. 5. Capable of detecting only SARS-CoV-2 Four (4) targets-RNase P, SARS-CoV-2, Influenza A and Influenza B. No ability to determine viability or quality of Utilizing RNase P, the viability and quality of specimen sample if home collection is a the specimen sample can be determined, which preferred method due to lack of RNase P. is extremely advantageous in home sample collection without proctoring the collection method.

Preferred embodiments are described in the following examples. Other embodiments within the scope of the claims herein will be apparent to one skilled in the art from consideration of the specification or practice of the invention as disclosed herein. It is intended that the specification, together with the examples, be considered exemplary only, with the scope and spirit of the invention being indicated by the claims, which follow the examples.

Example 1. Development of a Robust Test System for the Detection of Influenza A, Influenza B, and SARS-CoV-2 by Multiplex RT-PCR Introduction

An outbreak of pneumonia of unknown etiology in Wuhan City, Hubei Province, China was initially reported to WHO on Dec. 31, 2019. Chinese authorities identified a novel coronavirus (2019-nCoV), which has resulted in thousands of confirmed human infections in multiple provinces throughout China and many countries including the United States. Cases of asymptomatic infection, mild illness, and severe illness with an estimated 2.44-million deaths reported worldwide (Feb. 19, 2021, www.worldometers.info/coronavirus/).

In response to the COVID-19 pandemic, the CDC developed a singleplex RT-PCR assay for use in public health laboratories to detect the N1, N2, and N3 nucleoprotein sequences of COVID-19 (now referred to as SARS-CoV-2), and the p30 subunit of the human RNase P gene as a clinical sample control (Prevention, 2020). However, the CDC singleplex assay was not without limitations including contamination of the N3 primer/probe set leading to large number of inconclusive results (Willman, 2020) and the use of a singleplex assay which only allowed for 21 samples to be extracted and analyzed using a 96-well real-time instrument. The CDC dropped the contaminated N3 primer/probe set from the singleplex assay which increased the number of samples capable of being analyzed from 21 to 29 per run. However, early into the pandemic, it was realized that a singleplex assay approach was not feasible to test the sheer volume of specimens arriving at State Public Health Laboratories.

To increase extraction processes to enable laboratories to increase test capacity for SARS-CoV-2 testing, Thermo Fisher developed MagMax™ Viral and Pathogen Nucleic Acid Isolation Kits for use on the KingFisher Flex mangnetic particle processor to extract up to 96 specimens in 30-minutes. In addition, Thermo Fisher Scientific developed a multiplex RT-PCR assay for the detection of SARS-CoV-2 in clinical samples in response to the limitations of the CDC's singleplex assay and on Mar. 13, 2020, Thermo Fisher Scientific received EUA-approval by the Food and Drug Administration (FDA) for their TaqPath COVID-19 Combo Kit. The TaqPath COVID-19 Combo Kit contains exogenous extraction control reagents (MS2 phage), SARS-CoV-2 primers and probes, and the PCR master mix required to run the assay for detection of SARS-CoV-2 in clinical samples. Three individual primers and probe sets target ORF lab, ORFS (Nucleoprotein gene), and S (Spike glycoprotein gene) of SARS-CoV-2. In addition, the Combo Kit also contains primers and probe to detect MS2 phage RNA which is added to each sample prior to extraction to function as a metric for determining extraction success (Administration, 2020; Scientific, 2020).

However, despite the increased number of samples that the KingFisher platform could extract and the number of COVID-19 tests analyzed using the Combo Kit, multiple issues with the use of the testing process continued to provide significant challenges within the laboratory environment. First, the MS2 phage internal extraction control, is temperature sensitive, unstable, and demonstrated significant variability during extraction. The addition of exogenous extraction material (MS2 phage) provides no information surrounding the integrity of the specimen being extracted as no internal assessment of any human cell markers are available to verify human cells are present in the clinical sample. Second, high background noise associated with the lack of a passive-reference dye in the multiplex PCR mix leading to substantial variability in accurate analysis of sample amplification curves due to a wide signal-to-noise ratio (Scientific, 2020). Third, the TaqPath COVID-19 Combo Kit requires laboratory staff to perform several dilutions of the SARS-CoV-2 RNA template control for use as a PCR positive control. Stability and failures associated with dilutions of the COVID-19 Positive Template Control occur frequently leading to repeat testing, increased turn-around-time in test reporting, and increased accrued cost. Fourth, reagent cost and shortages have been a substantial issue during the pandemic. The cost for testing each sample for SARS-CoV-2 using Thermo Fisher reagents is ˜$3.18 per extraction and $15.98 for analysis by PCR for a total reagent test cost of ˜$19.60 per sample. Lastly, the TaqPath COVID-19 Combo Kit only tests for SARS-CoV-2 in clinical samples (Id.). However, infection with influenza presents with similar clinical manifestations and is equally as clinically devastating as SARS-COV-2 to the elderly and immunocompromised (Gooskins et al., 2009; Green and Beck, 2017; Li et al., 2009; Ljungman et al., 1993; Moghadami, 2017).

To this end, we developed a robust and cost-effective test method for the detection of influenza A, influenza B, and SARS-CoV-2 which uses a defined Non-Viral Extraction control, and a stable and defined Positive Template Control. In addition, clinical samples can be extracted on current KingFisher Flex platforms and analyzed on current real-time instruments. We describe herein the process for implementation and validation of the FluV19 Multiplex RT-PCR assay performed at Reditus Laboratories.

Results GRD Extraction Reagents are Equivalent to MagMax™ Viral/Pathogen Nucleic Acid Isolation Kits.

The current standards for nucleic acid extraction for detection of viral pathogens includes column-based manual extraction methods (Prevention, 2020; Prevention, 2021) and magnetic bead-based extractions on platforms (Scientific, 2020). Each of these extraction processes have proven track records in successfully extracting viral nucleic acids from clinical samples and have been approved for use in numerous laboratories for isolation of Influenza and SARS-CoV-2 from clinical samples (Prevention, 2020; Prevention, 2021; Scientific, 2020). However, limitations in the supply chain and the high cost of reagents have significantly impacted laboratories and their capacity to meet the needs of clinical testing of these pathogens.

To reduce the burden of reagent shortages and overall reagent cost, we investigated the possibility of developing cost-efficient extraction reagents to use on our laboratory's current KingFisher Flex extraction platforms to extract viral nucleic acids from clinical samples equivalent to the MagMax™ Viral/Pathogen Nucleic Acid Isolation Kit (MVP II) currently used within Reditus Laboratories for SARS-CoV-2 extraction.

The MagMax™ MVP II kit utilizes a combination of proteinase K digestion and guanidine thiocyanate (GTC) lysis buffer to degrade viral nucleoproteins and lyse cellular membranes to release nucleic acids which are then bound to magnetic beads and purified by the KingFisher platform. Specifically, during the extraction process outlined in the TaqPath COVID-19 EUA (Scientific, 2020), 265 μl of GTC-lysis buffer is added to 200 μl of specimen transferred into a 96-position deep well plate containing 5 μl of 20 mg/ml proteinase K (Id.). The specimen cocktail is then heated on the KingFisher platform at 65° C. for 5-minutes and mixed by the KingFisher platform. While proteinase K is efficient at cleaving peptide bonds and digestion of proteins, addition of high molar concentrations of GTC lysis buffer to specimens may inactivate proteinase K activity as guanidine thiocyanate is a strong protein denaturant (Lapanje, 1971; Stepanehko et al., 2012; Wingfeld, 2001). Therefore, we sought to formally test the hypothesis that particular extraction reagents (GRD) lacking proteinase K would work equivalent to the Thermo Fisher MagMax™ MVP II extraction process.

To test our hypothesis, a high-positive SARS-CoV-2 clinical sample previously extracted with MagMax™ MVPII extraction reagents on the KingFisher Flex and tested using the TaqPath COVID-19 Combo Kit was diluted in 0.5 log increments ranging from undiluted (10⁰) through 10⁻⁸ using a negative clinical sample as the diluent. This dilution series was based on a clinical sample which originally amplified each of the SARS-CoV-2 gene targets at: i. N-gene (Cq=12.5), ii. S-gene (Cq=12.9), iii. ORF lab (Cq=12.1). Thus, it was anticipated that at the terminal 10⁻⁸ dilution the specimen Cq values for each viral gene target should amplify at approximately 40 cycles and be beyond the limit of detection of the assay. Each dilution of sample beginning at 10^(−0.5) dilution was extracted on the KingFisher extraction platform simultaneously using either the MagMax™ MVPII (EUA-approved) or Reditus Extraction reagents (Laboratory Developed).

Specimens extracted with the MagMax™ MVP II extraction reagents were performed in accordance with the EUA-approved method using the MVP_2Wash_200_Flex program on the KingFisher extraction platform (Scientific, 2020). Specifically, 200 μl of each sample was added to each well of a 96 deep well plate containing 5 μl of MS2 phage exogenous extraction control and 5 μl of proteinase K. Following transfer, each sample received 275 μl of lysis reagents consisting of 265 μl of MagMax™ Binding Solution and 10 μl of MVP II binding beads. Samples were extracted and washed with 500 μl MagMax™ wash solution followed by wash in 1 ml of 80% ethanol and eluted in 50 μl of elution buffer.

Specimens extracted using Reditus extraction reagents (GRD) were also extracted on the KingFisher extraction platform using the MVP2_Wash_200_Flex program. For specimen extraction, a total of 280 μl of lysis reagents consisting of 265 μl of GRD Lysis Buffer (GRD-LB), 5 μl of MS2 Phage exogenous extraction control, and 10 μl of MVP II magnetic beads were added to each well of a 96-position deep well plate and 200 μl of each specimen dilution being dispensed directly into the lysis buffer. Following specimen transfer, magnetic bead binding was enhanced by transferring 640 μl of 80% Ethanol to each well. Samples were extracted and washed with 500 μl GRD wash buffer (GRD-WB) followed by wash in 1 ml of 80% ethanol and eluted in 50 μl of Reditus elution buffer (GRD-EB).

The isolated nucleic acid from each extraction process was amplified simultaneously using PCR reaction mix of the EUA-approved TaqPath COVID-19 Combo Kit™ (Id.) and amplified on a single reaction plate using a QuantStudio 12K Flex real-time instrument and analyzed using Applied Biosystems Design and Analysis Software. All data were analyzed and the mean±sem of n=3 replicates per specimen dilution are presented in FIGS. 5A, 5B, 5C and 5D.

Dilutions of the clinical specimen extracted using the MagMax™ extraction reagents demonstrated successful amplification of the SARS-CoV-2 N-gene target from 10^(−0.5) (Cq=14.32±0.007) through 10^(−6.0) (Cq=33.66±0.30) dilution with the anticipated ˜1.5 cycle difference between dilutions (FIG. 5A). MagMax™ was unable detect amplification of the N-gene beyond the 10^(−6.0) dilution (FIG. 5A). The same dilutions of clinical specimen extracted using GRD reagents detected SARS-CoV-2 N-gene amplification at equivalent cycles for each dilution (FIG. 5A). However, the range of detection for the N-gene for specimen dilutions extracted with GRD reagents also detected amplification of N-gene at the 10^(−6.5) dilution (Cq=36.25±1.05) which was not detected in the same specimen dilution extracted with MagMax™ reagents (FIG. 5A). These data suggest that the GRD extraction reagents, which lack the addition of proteinase K, do lead to a decrease in extraction efficiency to detect the SARS-CoV-2 N-gene in the same dynamic range of viral loads as the MagMax™ extraction reagents which require the addition of proteinase K.

Similarly, dilutions of the clinical specimen extracted using the MagMax™ extraction reagents demonstrated successful amplification of the SARS-CoV-2 S-gene target from 10^(−0.5) (Cq=14.52±0.012) through 10^(−6.0) (Cq=34.00±0.22) dilution with the anticipated ˜1.5 cycle difference between dilutions (FIG. 5B). MagMax™ was unable detect amplification of the S-gene beyond the 10^(−6.0) dilution (FIG. 5B). The same dilutions of clinical specimen extracted using GRD reagents detected SARS-CoV-2 S-gene amplification at equivalent cycles for each dilution (FIG. 5B). These data suggest that the GRD extraction reagents, which lack the addition of proteinase K, in the extraction efficiency to detect the SARS-CoV-2 S-gene in the same dynamic range of viral loads as the MagMax™ extraction reagents which require the addition of proteinase K.

For ORF lab amplification, GRD Reagents demonstrated successful amplification of ORF lab from 10^(−0.5) (Cq=15.41±0.20) through 10^(−6.0) (Cq=33.64±0.10) with the anticipated ˜1.5 cycle difference between dilutions (FIG. 5C). MagMax™ reagents demonstrated similar detection from 10^(−0.5) through 10^(−6.0) and at the additional 10^(−6.5) dilution (Cq=34.47±1.19) (FIG. 5C).

Lastly, the overall extraction efficiency of both extraction reagents was assessed by the amplification of the internal exogenous MS2 phage control which is added at equivalent volumes/concentrations to each specimen being extracted. At all dilutions (10^(−0.5) through 10^(−8.0)) both MagMax™ and GRD extraction reagents isolated equivalent MS2 phage from each specimen as indicated by a Cq<0.5 variation in MS2 amplification between each respective dilution. Thus, both MagMax™ and GRD reagents performed equivalently at extraction of the internal MS2 phage control (FIG. 5D).

While the additional dilution at 10^(−6.5) was detected by MagMax™ for ORF lab and the additional dilution at 10^(−6.5) was detected by GRD for N-gene, these did not impact the overall detection of any clinical specimen dilution by either extraction reagent. Specifically, positive identification of SARS-CoV-2 using the TaqPath COVID-19 Combo Kit™ relies on positive amplification for 2 of the 3 viral gene targets and the amplification of the internal MS2 phage internal control (Id.). Thus, both extraction reagents performed equivalently and were not statistically significant in the recovery and amplification of each viral- and control-targets at each dilution. These data suggest that the Reditus extraction reagents (GRD) used on the KingFisher Flex extraction platform may be used as a cost-effective alternative to commercially available MagMax™ extraction reagents.

Samples Extracted with GRD Reagents have Less Variability than MagMax™ Extraction.

The previous data suggest that both GRD and MagMax™ extraction reagents can recover equivalent amount of SARS-CoV-2 and MS2 phage RNA across an equivalent dynamic range of viral load from clinical specimens (FIGS. 5A, 5B, 5C and 5D). However, the reproducibility of extraction efficiency (i.e. variance) was not compared over time. To this end, an experiment was conducted to estimate the systematic measurement of error (i.e. bias) of GRD reagents relative to the EUA-approved MagMax™ extraction reagents.

To address the overall bias in extraction efficiency, n=5 independent clinical samples were identified which were previously reported as positive for SARS-CoV-2 and which amplified between 27 to 29 cycles for each of the viral gene targets using the TaqPath COVID-19 Combo Kit™. Over 5 Days, each specimen was extracted in triplicate using both GRD and MagMax™ methods and tested by RT-PCR using the TaqPath COVID-19 Combo Kit™. Thus, a Σ=75 data points were generated for each extraction method and the mean±sem for each data set per day, was analyzed and compared against the Day 0 (T₀) sample. The variation for each extraction method was assessed by analyzing each sample for the mean (x), stdev (σ), and sem (σ _(x) ) of each sample over the 5-Day period (FIGS. 6A, 6C, 6E, 6G). Each of the independent measurements per sample over 5-Days (Σ=75) also represents the statistical “true value (V_(T))” for each sample and was used to calculate the experimental bias (Vs) for both extraction process as defined by

$V_{B} = \frac{\sum\left\lbrack {{V_{E} - V_{T\; 1}},{V_{E} - V_{T\; 2}},{V_{E} - {V_{T\; 3}\mspace{14mu}\ldots\mspace{14mu} V_{E}} - V_{T\; 25}}} \right\rbrack}{DF}$

(CLSI, 2014; Owen and Chou, 1983; Yee, 1988).

Analysis of the overall mean (x), stdev (σ), and sem (σ _(x) ) of the Σ=75 data points collected from each of the viral targets and MS2 phage extraction control for the respective extraction process (MagMax™ vs. GRD) indicate that detection of viral gene target was equivalent between extraction reagents (FIGS. 6A, 6C, 6E, 6G). Specifically, analysis of N-gene amplification following MagMax™ extraction across n=5 Days demonstrated an average Cq=28.37±0.07 and an average Cq=28.79±0.68 by GRD extraction (FIG. 6A). Analysis of S-gene following MagMax™ extraction across all timepoints indicated an average Cq=29.36±0.64 amplification and Cq=30.07±0.91 following extraction with GRD reagents (FIG. 6C). Similarly, ORF lab amplified with an average Cq=28.39±0.62 after MagMax™ extraction and Cq=29.04±0.71 following GRD reagent extraction (FIG. 6E). Lastly, MagMax™ extraction reagents produced an average Cq=23.57±0.90 for amplification of MS2 phage across n=5 Days and an average Cq=23.17±0.08 following GRD extraction across the same timepoints and samples (FIG. 6G).

The experimental bias in each extraction process was analyzed using the data collected in FIGS. 6A, 6C, 6E and 6G and is presented in FIGS. 6B, 6D, 6F and 6H for each of the respective targets. Specifically, the initial amplification results for each sample represented the estimated expected value (V_(E)) using each test method and was compared to the error of each recurrent value over the 5-Days of analysis (refer to bias equation). Bias in an experimental system is related to the confidence interval of the coefficient in variation (CI) where bias ≤1 represents a highly unbiased system with a ˜99% CI. Experimental systems/assays which demonstrate 1<bias ≤3 indicate an unbiased system with a ˜95% CI. Any system where bias >3 indicates a biased system which falls below the 95% confidence interval indicating that the system contains bias and is unlikely to generate consistent results (CLSI, 2014; Owen and Chou, 1983; Yee, 1988).

When these metrics were applied to assess the overall bias in the extraction systems, samples extracted with MagMax™ reagents all fell within above the 95% confidence interval range for all viral and MS2 phage control targets amplified (N=1.58±0.08, CI=˜96.8%; S=1.30±0.63, CI=97.6%; ORFlab=2.17±0.06, CI=˜96.9%; MS2=1.26±0.09, CI=˜97.6%) (FIGS. 6B, 6D, 6F and 6H, respectively).

When the same analysis to estimate bias in specimens extracted with GRD reagents, the overall bias in extraction performance was significantly less following amplification all viral gene and control targets than observed by extraction with MagMax™ (FIGS. 6B, 6D, 6F and 6H, respectively). Specifically, reproducibility of amplification of N-gene was achieved with a CI=˜97.8% (1.06±0.06; FIG. 6B). Similarly, analysis of S-gene amplification reproducibility had a CI=˜99.0% (0.48±0.06; FIG. 6D) and ORF-lab demonstrated a CI=˜97.1% (1.58±0.7; FIG. 6F). Consistent with MagMax™ extraction, reproducibility of MS2 amplification using GRD reagents was equivalent to that of MagMax™ with an overall CI=˜97.6 (1.20±0.8; FIG. 6H).

The accumulation these data indicate that the Reditus extraction reagents (GRD) demonstrate equivalence in extraction efficiency on the KingFisher Flex magnetic particle processor as the MagMax™ commercial standard extraction reagents extracted on the same platform. This inference is based on the ability of GRD reagents to 1) accurately detect the each of the SARS-CoV-2 specimens at the same dilutions detected following extraction using the MagMax™ extraction reagents (FIGS. 5A, 5B, 5C and 5D) with less than a 1.5 cycle difference in amplification between comparable dilutions, and 2) decrease the overall extraction variability of extraction as determined through estimation of bias which tested the extraction efficiencies of both GRD an MagMax™ extraction reagents using the same n=5 specimens extracted and amplified over 5 Days (FIGS. 6A-6H). Thus, GRD reagents can be used in lieu of MagMax™ reagents for extraction of viral nucleic acids from clinical specimens for analysis by RT-PCR. Total Genomic RNA is Reliable and Robust for Use as a Non-Viral Control (NVC).

We were interested to expand testing of SARS-CoV-2 to include simultaneous testing for Influenza A and Influenza B in clinical specimens. Aside from the limitation that the COVID-19 Combo Kit™ only tests for SARS-CoV-2, a significant limitation of the COVID-19 Combo Kit™ for the detection of SARS-CoV-2 is addition of the MS2 RNA bacteriophage (phage) as exogenous extraction control in each sample being extracted. Federal clinical testing regulations require that each test system that has an extraction phase for analysis by molecular methods must contain at least two control materials: i) one that can detect errors in the extraction process, and ii. one for detecting errors in amplification (42 CFR 493.1256). While the MS2 phage extraction control provided as part of the TaqPath COVID-19 Combo Kit™ meets the requirements specified in 42 CFR 493.1256, amplification of MS2 phage RNA in each sample does not provide any indication in either the quality of the sample being tested, nor the accuracy of the test collection method being used. Specifically, samples which have not been properly collected may not have a sufficient number of human epithelial cells contained with the sample to accurately detect viral pathogens (i.e. SARS-CoV-2, Influenza, etc.). Likewise, specimens may be contaminated or contain inhibitors which can affect accurate detection by PCR.

The human ribonuclease protein (RNase P) is present in every human cell and is required for normal function of viable cells (Altman, 2011). The p30 subunit of the human RNase P gene is currently widely employed in numerous clinical molecular assays as an internal control to assess sample integrity while detecting analytes by molecular analysis and the primers and probes for these assays are well established (Prevention, 2021; Fernandes-Monteiro et al., 2015; Innings et al., 2007; Wozniak et al., 2020). Therefore, we were interested to explore the use of the p30 subunit of RNase P as an internal extraction control for the development of a multiplex RT-PCR assay. Since an extraction control must be present which can detect errors in the extraction process (42 CFR 493.1256) it would be possible to use diluted total human DNA in aqueous phase to include as a non-viral control (NVC) to be extracted alongside clinical specimens and analyzed by PCR using primers and probes to detect RNase P present in both the NVC and clinical specimens. Since the viral pathogens we were interested in developing an assay for are single-stranded RNA viruses (ssRNA), reverse transcription of the viral genomes (i.e. influenza, SARS-CoV-2) is used to convert viral RNA to cDNA for amplification by PCR. Thus, using total human DNA as a source of RNase P for a non-viral extraction control (NVC) would not assess the reverse transcriptase activity during RT-PCR. We hypothesized that human total genomic RNA could be used as the source of RNase P for a NVC as it would meet the control requirements specified within 42 CFR 493.1256 for extraction and amplification. We were interested in this possibility as an RNA RNase P control approach could also be used to define a specific concentration used in extraction to assess overall extraction efficiency based on the amplification profile of the RNA control material. To this end, we performed a series of tests to determine the best concentration of total human RNA for use which demonstrated consistent amplification values following extraction, and which determined the overall stability of the NVC over time.

Primer sequences for RNase P were obtained from the Center for Disease Control and Prevention (CDC) real-time Measles RT-PCR protocol (Prevention, 2021) and purchased through GenScript (Refer to Materials and Methods; SEQ ID NOs:1-10). Human total RNA control (50 ng/μl) was purchased from Applied Biosystems (Cat #4307281, Foster City, Calif.). Total control RNA was diluted to a starting concentration of 1.0 ng/μl in 10 mM Tris and serial diluted in a final volume of 1 ml at 0.5 log increments in Tris (pH 8.0) from 1.0 ng/μl to 0.0316 ng/μl. A total of 200 μl of each dilution was extracted in triplicate using GRD reagents on the KingFisher extraction platform and analyzed by RT-PCR on a QuantStudio 12K Flex real-time instrument using 5 μl of elution in a total reaction volume of 25 μl (Table 3). An amplification range of 28±2 cycles for RNase P was pre-established to: i) maximize the total number of NVC reactions capable of being generated from the stock 50 ng/μl, ii) establish a defined amplification range to monitor extraction efficiency, and iii) identify stability fluctuations during clinical implementation of the NVC.

TABLE 3 RNase P RT-PCR Reaction Mix Description 1x (μl) 10x (μl) 15x (μl) RNase P Fwd (9 μM) 0.54 5.4 8.1 RNase P Rvs (9 μM) 0.54 5.4 8.1 RNase P Probe (3 μM) 0.18 1.8 2.7 4X Fast Virus Enzyme 5.0 50.0 75.0 Mix Molecular Grade H₂O 8.74 87.4 131.1 Total Master Mix Volume 15.0 150.0 225.0

Analysis of extracted NVC by RT-PCR revealed an optimal concentration of total human control RNA for use as a non-viral extraction control between 0.31 ng/μl and 0.1 ng/μl (FIG. 7A). Specifically, a 200 μl extraction at 0.31 ng/μl total human control RNA amplified RNase P at 27.17±0.01 cycles and 200 μl extraction at 0.1 ng/μl amplified RNase P at 28.84±0.11 cycles (FIG. 7A). A 200 μl extraction at 0.031 ng/μl was too dilute to amplify RNase P within the pre-established range (Cq=30.35±0.14; FIG. 7A) and 200 μl extraction at 1.0 ng/μl was 10-fold more concentrated than required (Cq=25.09±0.15; FIG. 7A). However, since extraction at 1.0 ng/μl is at 10× concentration, these data also indicate that a 1.0 ng/μl stock of total human control RNA could be generated and stored in aliquots to preserve RNA integrity until such time to prepare a 0.1 ng/μl NVC 1× working stock (FIG. 7A).

A 200 μl extraction at 0.1 ng/μl was sufficient to amplify RNase P within the desired 28±2 cycle range (FIG. 7A). Therefore, we chose this concentration as it increased the number of non-viral controls (NVC) capable of being generated from a 50 ng/μl commercial stock. Therefore, a test was conducted to determine the stability of a 1× working NVC stock over time when stored at 2-8° C. To this end, 5 ml of 0.1 ng/μl total human control RNA was prepared in 10 mM Tris (pH 8.0) and distributed into n=18, 200 μl aliquots. Three (n=3) aliquots were immediately frozen at <−70° C. and were identified as time zero (T₀) to establish the baseline amplification of RNase P in the NVC preparation. The remaining n=15 aliquots were stored at 2-8° C. At 1, 4, 8, 12, and 24 hours post preparation, n=3 aliquots were frozen at <−70° C. Twenty-four hours (24 hrs) after the last sample was frozen, all aliquots were thawed, extracted together using GRD reagents on the KingFisher Flex extraction platform, and analyzed simultaneously by RT-PCR using the PCR reaction mix outlined in Table 4. As expected, analysis of the extracted n=3, To samples of 0.1 ng/μl generated amplification of RNase P at 28.08±0.15 cycles (FIG. 7B) and demonstrated no loss in amplification relative to fresh preparation and extraction (FIG. 7B). When stored at 2-8° C., no significant depreciation in amplification was observed at 1 or 4 hours (29.14±0.12; FIG. 7B) and only a 4-fold decrease in RNase P amplification was observed in NVC stored for 8 hours at 2-8° C. prior to extraction (Cq=29.22±0.05; FIG. 7B) and at 12 hours at 2-8° C. (Cq=29.94±0.14; FIG. 7B). Non-viral control stored for 24 hours at 2-8° C. followed by extraction demonstrated amplification of RNase P at 30.53±0.17 cycles representing a >6-fold loss of RNA integrity and fell outside the predefined acceptable range of amplification at 28±2 cycles. Therefore, these data indicate that non-viral control at a concentration of 0.1 ng/μl is stable for up to 12 hours at 2-8° C. (FIG. 7B).

TABLE 4 RNase P RT-PCR Reaction Mix Description 1x (μl) 10x (μl) 15x (μl) RNase P Fwd (9 μM) 0.54 5.4 8.1 RNase P Rvs (9 μM) 0.54 5.4 8.1 RNase P Probe (3 μM) 0.18 1.8 2.7 4X Fast Virus Enzyme 5.0 50.0 75.0 Mix Molecular Grade H₂O 8.74 87.4 131.1 Total Master Mix Volume 15.0 150.0 225.0

The Reditus FluV19 Probe Design is Equivalent to the CDC FLuSC2 Probe Design.

In addition to development of a non-viral extraction control which tests the reverse transcriptase enzyme activity for RT-PCR, a positive template control (PTC) is needed for PCR which verifies the activity of each primer and probe used for analyte detection as well as the activity of the polymerase during PCR amplification (42 CFR 493.1256). Thus, to expand testing capabilities to include testing for Influenza A and Influenza B, we developed a plasmid containing viral sequence regions targeted by each of the CDC's primer and probe sets and which also contains the targeted gene sequence for the p30 subunit of the Human RNase P gene (FIG. 3; Materials and Methods). We favored the development of this control approach as current positive controls for the CDC FLuSC2 (Prevention, 2021) and other similar assays which test for Influenza A/B/SARS-2 utilize RNA as the positive template control for PCR (Scientific, 2021). These positive control strategies have demonstrated instability and inconsistencies leading to unnecessary repeat testing and are cumbersome in technical preparation for laboratorians as they require several dilution steps needed to generate the final control (Scientific, 2020, 2021; Prevention, 2021). In contrast, the use of a plasmid control approach allows for large-scale production of control template which is stable at multiple temperature ranges (2-8° C., −15±5° C., <−70° C.) for extended periods of time with no loss in amplification efficiency due to degradation (Brunet et al., 2017; Driessen et al., 2017). Additionally, bacteria transformed with control plasmid offers an endless supply of reagent and more than 1-million reactions of PTC can be generated with a single miniprep of plasmid in 50 μl elution. Lastly, plasmid control concentrations can be quantified by spectrophotometry and diluted to a defined range for both reproducibility and to also provide a relative copy number of genome equivalents for each gene target. Thus, the use of a plasmid control could be used for semi-quantitative PCR to identify the relative viral load within a patient specimen for each of the analytes tested.

To make the current CDC FluSC2 probe sets (Prevention, 2021) more-robust as a multiplex assay for use on real-time instruments, we modified the fluorophore and quencher combinations for use with the Fast Virus 1-Step Master Mix which contains ROX as a passive reference (SEQ ID NOs:15-18; Table 5) to reduce background noise associated with numerous assays lacking a passive reference in their PCR reaction mix. To validate our new probe/quencher combinations, we simultaneously tested our multiplex assay against the CDC FluSC2 assay using dilutions of our purified, linearized pMK-FluV19 control to determine the relative limit of detection and amplification efficiency of each of the assays. Specifically, 41 ng/μl of pMK-FluV19 was diluted serially in 0.5 log increments to a final dilution of 10⁻⁹ dilution with a terminal estimated genome equivalent 1.4×10° copies of influenza A, influenza B, SARS-CoV-2, and RNase P and 5 μl of each dilution was tested in triplicate by PCR using the CDC's reaction formulation (Prevention, 2021) and by the FluV19 reaction mix listed in Table 5. Data were analyzed using Applied Biosystems Design & Analysis software for each PCR reaction and the mean±sem of each dilution, by analyte, was calculated and graphed using GraphPad Prism software (FIG. 8).

TABLE 5 Reditus FluV19 Multiplex RT-PCR Reaction Mix Description 1x (μl) 10x (μl) 100x (μl) Component B 2.4 24 240 (combined primer mix) Component C 2.4 24 240 (combined probe mix) 4X Fast Virus Enzyme 5.0 50 500 Mix Molecular Grade H₂O 5.2 52 520 Total Master Mix Volume 15.0 150 1,500

Analysis of data indicated that both the CDC PCR formulation and the modified Reditus PCR formulation demonstrated equivalent detection of all viral- and control gene-targets (FIGS. 8A, 8B, 8C and 8D). Specifically, both the CDC FLuSC2 and Reditus FluV19 assays were able to detect equivalent N-, S-, and ORF lab-gene copies at 10⁻⁸ dilution of linearized plasmid representing an estimated limit of detection at ˜130 genome copy equivalents (FIGS. 8A, 8B and 8C). Likewise, detection of RNase P using linearized plasmid was also equivalent between test methods with terminal detection at 10^(−8.5) dilution representing ˜42 gene copy equivalents (FIG. 8D). Interestingly, when a similar experiment was performed using dilutions of circularized pMK-FluV19, both assays detected Influenza A and Influenza B targets at equivalent genome equivalents of ˜130 copies; however, detection of SARS-CoV-2 N-gene increased an additional 5-fold with an overall limit of detection of ˜20 genome copy equivalents (data not shown). The decrease in detection using linearized pDNA may have resulted from restriction enzyme star activity within the pMK-FluV19 SARS-CoV-2 sequence. Thus, the estimated limit of detection for each analyte is ˜130 genome equivalents for influenza A and influenza B, ˜60 genome equivalents for SARS-CoV-2, and ˜42 gene equivalents for RNase P. In short, neither the modifications in fluorophore/quencher combinations or the change in Master Mix formulation of the Reditus FluV19 assay reduced detection relative to the EUA-approved CDC FLuSC2 assay.

Analysis of the Complete Fluv19 Assay Performs Equivalent to the CDC FluSC2 Assay and Better than the Commercial Thermo Fisher TaqMan COVID-19 Flu AB Assay.

The accumulation of data thus far indicate that Reditus extraction reagents (GRD) are equivalent to Thermo MagMax™ MVP II extraction of clinical samples on the KingFisher Flex extraction platform (FIG. 5) but demonstrate less variability than MagMax™ extractions over time (FIG. 6). Additionally, we demonstrate the 0.1 ng/μl of total human genomic RNA control is stable for 12 hours at 2-8° C. and can be used successfully as a non-viral (NVC) control reagent to test for reverse transcriptase activity during RT-PCR following extraction (FIG. 7). Lastly, we confirmed that the combination of modified CDC probe sequences for influenza A, influenza B, and SARS-CoV-2 and Fast Virus Enzyme containing ROX performs equivalently to the EUA-approved CDC primer and probe set in detecting the same genome copy equivalents of influenza A, influenza B, SARS-CoV-2, and RNase P (FIG. 8). We next sought to test the combined Reditus FluV19 assay using GRD extraction reagents and FluV19 RT-PCR multiplex using a 200 μl of clinical samples containing influenza A, influenza B, SARS-CoV-2, and combinations thereof, to detect both individual and co-infections. To fully vet the FluV19 assay, we also tested the same samples extracted using 200 μl of specimen with MagMax™ MVPII and tested either using the CDC FLuSC2 assay (Prevention, 2021) or using the TaqMan COVID-19 FluA,FluB Multiplex Assay (Cat #A47701, Thermo Fisher, Waltham, Mass., Scientific, 2021).

Analysis of PCR results demonstrated equivalence in detection of Influenza A single-positive clinical specimens extracted and tested with either the CDC FLuSC2 RT-PCR assay or the Reditus FluV19 assay (FIG. 9A). The same clinical sample was not-detected by either the FLuSC2 or the FluV19 assay but was detected with the TaqMan COVID-19 FluA,FluB Multiplex Assay, albeit at a Cq value higher than the 38 cycle cut-off used for the FLuSC2 and FluV19 assays. A separate clinical sample (A-08316; FIG. 9A) was undetected by the Thermo TaqMan assay but was detected at equivalent cycles (Cq=37) by both FLuSC2 and FluV19 assays (FIG. 9A). In contrast, the Thermo TaqMan COVID-19 FluA/B produced n=5 false-positive results which were discordant to both the FLuSC2 and FluV19 assays and the expected results provided by IDPH-Springfield and NorthShore University HealthSystem. The high false-positive detection of Influenza A is likely due to differences in primer and probe sets of the Thermo TaqMan assay, but this cannot be confirmed as the targets of their sequences are proprietary. Analysis of single-positive Influenza B specimens indicated that all appropriate specimens were detected regardless of assay (FIG. 6B). Likewise, analysis of all single-positive SARS-CoV-2 clinical specimens were equivalently detected across each extraction method and RT-PCR assay (FIG. 9C).

When combinations of clinical specimens were tested, the Reditus FluV19 assay was accurate in detecting 100% of all specimens for containing influenza A (n=48), influenza B (n=48), and SARS-CoV-2 (n=32), regardless of concentration (FIGS. 10A, 10B, 11A, 11B, 12A, 12B, 13A, 13B and 13C). Likewise, all influenza A-positive specimens were also detected successfully when tested with the Thermo TaqMan assay (FIG. 10A, 11A, 13A). In contrast, n=1 specimen (AL-BL-4), containing low amounts of influenza A (AL), was undetected by the CDC FLuSC2 assay (FIG. 10A). We were concerned that this might have represented a missed sample extraction leading to the false-negative result by the FLuSC2 assay. However, as anticipated, AL-BL-4 was positive for influenza B by the CDC FLuSC2 assay (FIG. 10B) and RNase P (not shown). Thus, these data indicated that the specimen AL-BL-3 was extracted with sufficient viral RNA and represented a single false-negative result for the CDC FluSC2 assay (FIG. 10A, 11A, 13A). All specimens analyzed for the detection of Influenza B were consistently detected in samples containing either high (BH) and low (BL) amounts of Influenza B, regardless of test method used (FIG. 10B, 12B, 13B). Likewise, all specimens analyzed for the detection of SARS-CoV-2 were consistently detected in samples containing either high (BH) and low (BL) amounts of SARS-CoV-2, regardless of test method used (FIG. 11B, 13B, 13C).

Neither the FluV19 or FLuSC2 assays had any false-positive influenza A detection in any negative specimens with an overall analytical sensitivity of 98.6%, 100% overall specificity and precision (Table 6). In contrast, the Thermo TaqMan COVID-19 FluA/B produced 5 influenza A false-positive results which were discordant to FLuSC2 and FluV19. This led to an overall reduction in sensitivity (98.6%), specificity (92.3%), and precision (93.2%) of the Thermo TaqMan assay to detect influenza A in clinical samples (Table 6). When the accuracy of detecting influenza A in clinical samples was calculated, the Reditus FluV19 assay was 99.2% accurate, the CDC FLuSC2 assay was 98.5% accurate, and the Thermo TaqMan assay was 95.6% accurate in detecting influenza A (Table 10). While all the extraction methods/reagents and RT-PCR assays tested met the ≥95% accuracy standard for clinical use, the Reditus FluV19 assay demonstrated the greatest sensitivity and accuracy for detecting Influenza A in clinical samples (Table 6).

TABLE 6 Analytical Statistics Thermo Fisher Reditus CDC COVID19 FluV19 FLuSC2 FluA/B Influenza A # True Positives (a) 69 69 69 # False Positives (c) 0 0 5 # True Negatives (d) 60 60 60 # False Negatives (b) 1 2 1 Sensitivity [a/(a + b)] 98.6% 97.2% 98.6% Specificity [d/(c + d)] 100.0% 100.0% 92.3% Precision [a/(a + c)] 100.0% 100.0% 93.2% Accuracy [(a + d)/(a + b + c + d) 99.2% 98.5% 95.6% Influenza B # True Positives (a) 67 67 67 # False Positives (c) 0 0 0 # True Negatives (d) 69 69 69 # False Negatives (b) 0 0 0 Sensitivity [a/(a + b)] 100.0% 100.0% 100.0% Specificity [d/(c + d)] 100.0% 100.0% 100.0% Precision [a/(a + c)] 100.0% 100.0% 100.0% Accuracy [(a + d)/(a + b + c + d) 100.0% 100.0% 100.0% SARS-CoV-2 # True Positives (a) 55 55 55 # False Positives (c) 0 0 1 # True Negatives (d) 69 69 69 # False Negatives (b) 0 0 0 Sensitivity [a/(a + b)] 100.0% 100.0% 100.0% Specificity [d/(c + d)] 100.0% 100.0% 98.6% Precision [a/(a + c)] 100.0% 100.0% 98.2% Accuracy [(a + d)/(a + b + c + d) 100.0% 100.0% 99.2%

All extraction methods/reagents and RT-PCR assay tested were successful in extracting and detecting 100% of clinical samples containing Influenza B (Table 6). Therefore, the overall sensitivity, specificity, precision, and accuracy were 100% for all methods in detecting Influenza B in clinical samples (Table 6).

However, only the Reditus FluV19 and CDC FLuSC2 assays were able to accurately detect all specimens containing SARS-CoV-2 with no false-negative or false-positive results (Table 10). Thus, the overall sensitivity, specificity, precision, and accuracy was 100% for FluV19 and FLuSC2 methods to detect SARS-CoV-2 in clinical samples (Table 6). In contrast, the Thermo TaqMan assay generated n=1 false-positive result for SARS-CoV-2 in all the samples tested which resulted in a specificity and precision of 98.6% and an overall accuracy of 99.2% in detecting SARS-CoV-2 (Table 6).

The culmination of these data indicates that MagMax™ MVPII extraction on the KingFisher extraction platform coupled with detection using either the CDC FLuSC2 or Thermo COVID-19 FluA/B RT-PCR assays are sufficient in detecting ≥95% of all clinical specimens containing Influenza A, Influenza B, or SARS-CoV-2 (Table 6). However, greater sensitivity and accuracy in detecting Influenza A, Influenza B, and SARS-CoV-2 is achieved when clinical samples are extracted using Reditus extraction reagents (GRD) followed by RT-PCR analysis using the Reditus FluV19 assay (Table 6).

Discussion

The FluV19 RT-PCR Assay is More Accurate in Detecting Influenza a than the CDC FluSC2 Assay and Thermo Fisher TaqMan COVID-19 FluA/B RT-PCR Assays.

Extraction using GRD reagents are equivalent to MagMax™ Viral and Pathogen Nucleic Acid Isolation Kits (FIGS. 5A-5D) and demonstrate greater reproducibility and less overall variance (FIGS. 6A-6H). In addition, the Reditus FluV19 RT-PCR assay demonstrates and equivalent limit of detection as the EUA-approved CDC FLuSC2 assay (FIGS. 8A-8D). However, the combined GRD extraction and FluV19 RT-PCR reagents are combined, the Reditus Laboratory Developed Test (LDT) demonstrates greater accuracy in Influenza A detection (99.2%) than either the CDC FLuSC2 assay (98.5%) or the Thermo COVID-19 FluA/B assays (95.6%) when extracted using MagMax™ Viral and Pathogen Nucleic Acid Isolation Kits (Table 6). Additionally, the Reditus LDT demonstrates greater accuracy (100%) in detecting SARS-CoV-2 than the TaqPath COVID-19 FluA/B assay (99.2%) (Table 6). It is likely that the decrease in extraction variability using GRD reagents contributed to an overall increase in detection using the FluV19 RT-PCR assay for Influenza A and SARS-CoV-2 (FIGS. 6A-6H).

Extraction and Amplification Controls with the FluV19 Assay are Defined and More Reproducible than Other Assays.

As stated earlier, current extraction processes using MS2 phage as an exogenous control does not offer any information with regards to clinical specimen integrity. In contrast, RNase P can be used to determine whether human cells are present within the clinical sample and thus, sample collection was performed sufficiently enough to increase the likelihood of detecting influenza A, influenza B, and/or SARS-CoV-2 in a patient. Thus, the use of defined concentrations of total human control RNA as a non-viral control (NVC) which is extracted alongside clinical specimens is an excellent method to assess extraction efficiency and reverse transcriptase activity of the RT-enzyme. Coupled with the use of the pMK-FluV19 positive template control (PTC), the combined NVC and PTC assess all aspects of extraction and PCR by assessing RT activity, polymerase activity, and the functionality of each primer and probe set contained within the PCR reaction mix. Lastly, the technical ease by laboratory testing staff is greatly enhanced using the NVC and PTC reagents as no dilutions need to be performed prior to use during extraction and/or PCR but is not the case using either the CDC-FLuSC2, Thermo TaqpPath COVID-19 (Prevention, 2021), or Thermo TaqMan COVID-19 FluA/B assays (Scientific, 2021). Thus, the Reditus FluV19 assay is not only less variable and more accurate (FIGS. 6A-6H, Table 6) but is also easier for laboratory staff to perform.

Extraction with GRD Reagents and FluV19 is More Cost-Effective than MagMax™ Extraction Reagents and Detection Using the TaqPath COVID-19 Combo Kit.

Lastly, the cost for testing each sample for SARS-CoV-2 using Thermo Fisher MagMax™ reagents is ˜$3.18 per extraction and $15.98 for analysis using Thermo Fisher TaqPath COVID-19 RT-PCR assay for a total reaction cost of $19.60 per sample. In contrast, the cost to extract each clinical specimen using Reditus Extraction Reagents (GRD) is ˜$0.50 and ˜$4.00 using the FluV19 RT-PCR assay. Thus, the total cost savings per reaction using GRD extraction and the FluV19 RT-PCR assay is 15.10 per reaction. For a lab performing 2,000 reactions per day, the combined savings over the MagMax and TaqPath COVID-19 Combo Kit amounts to an $29,000 per week. In addition to the cost savings alone, the FluV19 Combo Kit can be used to detect SARS-CoV-2, Influenza A, and Influenza B in clinical samples.

Concluding Remarks

Reditus extraction reagents (GRD) combined with the FluV19 RT-PCR assay is a robust process for detecting Influenza A, Influenza B, and SARS-CoV-2 in clinical samples while simultaneously assessing sample integrity of specimens being tested. The cost of reagents to run each specimen is significantly reduced and increases the overall detection accuracy of each viral analyte. The controls established in the FluV19 assay offer a robust method for assessing quality control of each process in the testing method, offer greater reproducibility, and less effort in preparation than other available assays. Thus, the GRD FluV19 assay is a reliable and cost-effective assay for use in clinical laboratories to detect Influenza A, Influenza B, and SARS-CoV-2 in clinical samples.

Materials and Methods Preparation of Laboratory Reagents

1 Molar Tris (pH 8.0): 121.1 grams of Tris Base (CAS 77-86-1) was dissolved in 800 ml of distilled water (dH₂O). The pH of the mixture was adjusted to 8.0 using 1N HCL (CAS 7647-01-0,7732-18-5) and brought to a final volume of 1 L with dH₂O. The completed 1M Tris solution was sterilized by 0.22 μm filtration.

0.5 Molar EDTA (pH 8.0): 186.1 grams of Ethylenediaminetetraacetic acid (EDTA; CAS 60-00-4) was fully dissolved in 800 ml of dH₂O. The pH of the solution was adjusted to 8.0 using freshly prepared 5M Sodium Hydroxide (NaOH; 1310-73-2,497-19-8) and brought to a final volume of 1 L with dH₂O. The completed 0.5 M EDTA solution was sterilized by autoclaving for 15-minutes at 121° C.

0.5 Molar Urea: 30 grams of Urea (CAS 57-13-6) was dissolved in 800 ml of dH₂O and brought to a final volume of 1 L with dH₂O. The completed 0.5M Urea solution was sterilized by 0.22 μm filtration.

0.5% Bromophenol Blue: 5 grams of Bromophenol Blue (CAS 115-39-9) was suspended in 800 ml of dH₂O until homogenous. The mixture was brought to a final volume of 1 L with dH₂O.

Preparation of the GRD Lysis Buffer (GRD-LB; Alternatively Abbreviated as ReX-LB in U.S. Provisional Application No. 63/188,318, Filed May 13, 2021 and U.S. Nonprovisional Application Ser. No. 17/560,573, Filed Dec. 23, 2021)

200 ml of dH₂O was pre-heated to 67±3° C. on a heating stir-plate with stir bar, and the following Prepared Laboratory Reagents were added in sequential order: i. 50 ml of 1M Tris (pH 8.0), ii. 50 ml of 0.5M EDTA (pH 8.0), iii. 20 ml of 0.5M Urea, and iv. 20 ml of 0.5% Bromophenol Blue. To the mixture, 30 ml of Triton X-100 (CAS 9002-93-1) was added using a graduated serological pipettor and mixed by stirring until homogenous. Gradually, 472.8 grams of Guanidine Thiocyanate was added to the combined solution, mixed until thoroughly dissolved, and brought to a final volume of 1 L using dH₂O. The final concentrations of each component of the GRD Lysis Buffer (GRD-LB) are: Tris (pH 8.0, Cf=50 mM); EDTA (pH 8.0, Cf=25 mM); Triton X-100 (3% v/v); Urea (Cf=10 mM); Bromophenol Blue (Cf=0.01% v/v); and Guanidine Thiocyanate (Cf=4M).

Preparation of the GRD Wash Buffer (GRD-WB; Alternatively Abbreviated as ReX-WB in U.S. Provisional Application No. 63/188,318, Filed May 13, 2021 and U.S. Nonprovisional Application Ser. No. 17/560,573, Filed Dec. 23, 2021)

50 ml of dH₂O was pre-heated to 67±3° C. on a heating stir-plate with stir bar, and the following Prepared Laboratory Reagents were added in sequential order: i. 9.9 ml of 1M Tris (pH 8.0), and ii. 15 ml of 0.5M EDTA (pH 8.0). Gradually, 212.7 grams of Guanidine Thiocyanate was added to the combined solution, mixed until thoroughly dissolved and brought to a final volume to 300 ml with dH₂O. The GRD Wash Buffer (GRD-WB) was brought to a final volume of 1 L with 700 ml of 100% USP-grade Ethanol (CAS 64-17-5). The final concentrations of each component of the GRD-WB are: Tris (pH 8.0, Cf=10 mM); 0.5M EDTA (pH 8.0, 7.5 mM); Guanidine Thiocyante (1.82 M); Ethanol (Cf=70%).

Preparation of the GRD Elution Buffer (GRD-EB; Alternatively Abbreviated as ReX-EB in U.S. Provisional Application No. 63/188,318, Filed May 13, 2021 and U.S. Nonprovisional Application Ser. No. 17/560,573, Filed Dec. 23, 2021)

Preparation of the GRD-EB consisted of adding 10 ml of 1M Tris (pH 8.0) and 2.0 ml of 05M EDTA (pH 8.0) to 88.0 ml of dH₂O. The final GRD-EB solution was filter sterilized by 0.2 μm filtration. The final concentrations of each component of the GRD-EB are: Tris (pH 8.0, Cf=100 mM); EDTA (pH 8.0, 10 mM).

Primers and Probes

The sequences of influenza A, influenza B, SARS-CoV-2, and RNase P were taken directly from the Center for Disease Control and Prevention (CDC) Research Use Only (RUO) FluSC2 multiplex assay (SEQ ID NOs:1-8, 13, 14) (Prevention, 2021). However, the probe fluorophore and quencher designs were modified for use on real-time instruments to promote increased detection wider separation of fluorophore reporters and quencher design minimize crossover (SEQ ID NO:15-18). Additionally, the use of the TaqMan Fast Virus 1-Step Master (ThermoFisher Scientific, Cat 4444434) is specially formulated for use with multiplex RT-PCR assays from a range of specimen types, has been optimized to work under a range of common PCR-inhibitors, and contains ROX as a passive-reference dye which functions as a basis for normalization to eliminate detection of crossover fluorescence by the molecular platform (Biosystems, 2010). FluV19 primers and probes were purchased from GenScript® Biotech (Piscataway, N.J.) using the sequences and fluorophore/quencher combinations (SEQ ID NOs:1-20).

Additionally, CDC FLuSC2 primers and probes were also purchased from Integrated DNA Technologies (Coralville, Iowa) for use as a comparator against the modified probe fluorophore/quencher design.

PCR Enzymes Mix Reagents

The TaqPath 1-Step Multiplex Mix without ROX (A28523) for testing of the CDC FLuSC2 assay was purchased from Applied Biosystems and the preparation for the master mix can be found at Prevention, 2021.

The TaqMan™ Fast Virus 1-Step Master Mix with ROX (4444434) used with the Reditus FluV19 RT-PCR assay was purchased from Applied Biosystems. The preparation for the master mix is indicated in Table 3 and Table 5.

In Silico Analysis of Viral Core Sequences for Development of a Positive Template Control

The pMK-FluV19 positive control plasmid contains core sequences of: i) influenza A Matrix 1 protein (M1), ii) influenza B non-structural protein (NS1), iii) SARS-CoV-2 Nucleoprotein (N), and iii) Human RNase P (RP). To identify the core sequences of each pathogen target needed to produce a positive amplification profile, Geneious Prime® 2021.0.3 was used to perform a MAAFT alignment of target gene sequences for each of the viral pathogens to identify the core-sequence to integrate into the positive control plasmid herein referred to as pMK-FluV19.

For influenza A, 32,955 sequences of the matrix 1 (M1) gene were obtained from the NIAID Influenza Research Database (IRD) (Zhang et al., 2017) and were aligned against the curated primer and probe sequences (Prevention, 2021). While several minor C-A/A-C mismatches were identified within the primer and probe sequences of the M1 gene this did not significantly affect positive amplification (Stadhouders et al., 2010). Thus, sequence alignment indicated that the core sequence would provide detection of approximately ≥90% of all influenza A viruses by RT-PCR analysis. However, it remains possible that future mutations within the influenza B NS1 gene may affect detection of variants.

Similarly, 11,648 sequences of Influenza B Non-structural protein (NS1) were obtained from the NIAID Influenza Research Database (IRD) (Zhang et al., 2017) and were aligned against the curated primer and probe sequences (Prevention, 2021). As with alignment of influenza A primer/probe sets, no significant discrepancies in primer/probe binding were observed leading to a failure in detection of influenza B. Therefore, sequence alignment indicated that the cores sequence would provide detection of approximately ≥90% of all influenza B viruses by RT-PCR. However, it remains possible that future mutations within the influenza B NS1 gene my affect detection of variants. Data was obtained from the NIAID Influenza Research Database (IRD) (Zhang et al., 2017).

The 13,099 nucleotides of the SARS-CoV-2 Nucleoprotein (N) gene were obtained from the NIAID Virus Pathogen Database and Analysis Resource (ViPR) (Pickett et al., 2012) through the web site at www.viprbrc.org. Alignment of the N-gene sequences with the curated CDC primers and probe (Prevention, 2021) indicated that ≥95% of all SARS-CoV-2 N-gene sequences should be detected by RT-PCR using the current primer probe sequences with minor C/T substitutions within the forward primer and probe sequences that should not affect detection (Stadhouders et al., 2010). However, it remains possible that future mutations within the N-gene my affect detection of variants.

Use of Total Human Control RNA as a Non-Viral Extraction Control (NVC)

Human total RNA control (50 ng/μl) was purchased from Applied Biosystems (Cat #4307281, Foster City, Calif.). Total control RNA was diluted to a starting concentration of 1.0 ng/μl in 10 mM Tris (pH 8.0) and serial diluted in a final volume of 1 ml at 0.5 log increments in Tris (pH 8.0) from 1.0 ng/μl to 0.0316 ng/μl. A total of 200 μl of each dilution was extracted in triplicate using GRD reagents on the KingFisher extraction platform and analyzed by RT-PCR on a QuantStudio 12K Flex real-time instrument using 5 μl of elution in a total reaction volume of 20 μl (Table 4).

Development of pMK-FluV19 Positive Template Control (PTC)

The core sequences of Influenza A (M1), Influenza B (NS1), SARS-CoV-2 (N), and Human RNase P developed by in silico analysis were constructed using Geneious Prime® 2021.0.3 software. Leader and flanking sequences for each viral and human target gene were incorporated along with unique restriction sites for post-synthesis digest and analysis and for subcloning of additional/alternate gene products for future use (FIG. 4B). The total sequence presented in FIG. 4B was synthesized by GeneArt Gene Synthesis from Invitrogen (Thermo Fisher Scientific) in pMK-T backbone containing a Kanamycin resistance marker (FIG. 4A). The final construct was verified by sequencing and demonstrated 100% sequence identity of the insertion site.

Lyophilized pMK-FluV19 plasmid was resuspended at a concentration of 5 ng/μl in sterile 10 mM Tris (pH 8.0) and 1 μl of pDNA was used to transform competent DH5α E. coli for 20-minutes on ice. DH5α cells were heat-shocked at 42° C. for 40-seconds, placed on ice for 2-minutes, and 1 ml of sterile nutrient-rich Tryptic Soy Broth (TSB) for 1-hour prior. A total of 200 μl of transformed bacteria were plated on Tryptic Soy Agar plates containing 66 μg/ml of Kanamycin to preferentially enrich for E. coli containing the pMK-FluV19 vector. Isolated colonies were identified and enriched overnight in TSB containing 66 μg/ml Kanamycin and plasmid DNA was extracted using the A7510 Wizard® Plus Miniprep DNA Purification System (Promega, Madison, Wis.). One microgram (1 μg) of plasmid DNA was digested with SpeI, KpnI, and XbaI to verify successful transformation. A single isolate was selected which contained a 2,461 bp fragment (KpnI/XbaI), 279 bp fragment (SpeI/KpnI), and a 156 bp fragment (XbaI/SpeI). The selected isolate was cultured in TSB containing 66 μg/ml Kanamycin until log-phase growth was achieved. A glycerol stock of the cultured isolate was prepared by transferring 1 ml of log-phase culture into 427 μl of sterile 50% glycerol. The glycerol stock was maintained at ≤−70° C. for long-term storage.

Estimated Limit of Detection (LOD)

The estimated limit of detection (LOD) was established using linearized pMK-FluV19 plasmid. Specifically, 40 μg of pMK-FluV19 was linearized by digesting with 600 units of KpnI enzyme in CutSmart® buffer (New England Biolabs®) for 4 hours at 37° C. Complete digestion of pMK-FluV19 was confirmed by gel electrophoresis. Linearized pMK-FluV19 was purified overnight at −20° C. in 70% ethanol containing 8.3 mM EDTA and 0.17 M ammonium acetate (NH₄OAc) and collected by centrifugation at 21,000×g for 15-minutes at 4° C. Linearized pMK-FluV19 was washed with cold 70% ethanol to remove salts and the resulting pellet was dried and re-suspended in 40 μl of RNase-free 10 mM Tris (pH 8.0). The linearized pMK-FluV19 was centrifuged at 21,000×g for an additional 15-minutes to remove precipitated KpnI. A total of 19.8 of linearized pMK-FluV19 was purified as identified by spectrophotometry using a NanoDrop Onec (Thermo Fisher Scientific, Waltham, Mass.).

Linearized pMK-FluV19 was diluted to a starting concentration of 41 ng/μl and diluted in 0.5 log increments to a final concentration 4.10×10⁻⁸ ng/μl (i.e. 10⁰ to 10⁻⁹). Thus, the copies of viral gene targets being tested ranged from an estimated 1.38×10¹⁰ to 1.4×10° target equivalent/W. A total of 5 μl of each dilution was tested in triplicate by real-time PCR using the CDC FluSC2 multiplex assay as outlined in Prevention, 2021, and by the Reditus FluV19 RT-PCR multiplex (Table 5).

Clinical Validation Specimens

influenza A and influenza B clinical specimens used for validation of the Reditus FluV19 RT-PCR assay were obtained from the courtesy of Katie Caldwell at the Illinois Department of Public Health (Springfield, Ill.) and from courtesy of Matt Charles at NorthShore University HealthSystem (Evanston, Ill.). Previously reported SARS-CoV-2 negative positive clinical specimens were retained by Reditus Laboratories from prior analysis using the Thermo Fisher TaqPath COVID-19 Combo Kit. Negative clinical specimens were independently confirmed to be Influenza A and Influenza B negative using both the Reditus FluV19 and CDC FLuSC2 primer and probe sets.

To represent dual infection scenarios, combination-positive specimens were generated by diluting high-positive (low Cq value) Influenza A, Influenza B, and SARS-CoV-2 specimens using negative specimens as the diluent to achieve high (H) and low (L) combinations for each of the following scenarios:

Sample ID Analyte 1 Analyte 2 Analyte 3 AH-BH Influenza A Influenza B — High High AH-BL Influenza A Influenza B — High Low AH-CH Influenza A SARS-CoV-2 — High High AH-CL Influenza A SARS-CoV-2 — High Low BH-CH Influenza B SARS-CoV-2 — High High BH-CL Influenza B SARS-CoV-2 — High Low AL-BH Influenza A Influenza B — Low High AL-BL Influenza A Influenza B — Low Low AL-CH Influenza A SARS-CoV-2 — Low High AL-CL Influenza A SARS-CoV-2 — Low Low BL-CH Influenza B SARS-CoV-2 — Low High BL-CL Influenza B SARS-CoV-2 — Low Low AH-BH-CH Influenza A Influenza B SARS-CoV-2 High High High AH-BH-CL Influenza A Influenza B SARS-CoV-2 High High Low AL-BL-CH Influenza A Influenza B SARS-CoV-2 Low Low High AL-BL-CL Influenza A Influenza B SARS-CoV-2 Low Low Low

Equipment, Software, and Analysis

RT-PCR analysis was conducted using QuantStudio 12K Flex Real-Time molecular platforms (Carlsbad, Calif.). Instruments were calibrated for each of the fluorescent dyes used for detection of specific targets. Analysis of run data was performed using Applied Biosystems Design & Analysis Software version 2.4.0 (Thermo Fisher Scientific, Waltham, Mass.)

Bioinformatics and sequence analysis was performed using Geneious Prime Software version 2021.0.3 (Biomatters Ltd., San Diego, Calif.). Sequence alignments were performed in Geneious Prime using the MAFFT Alignment v.7.450 as described inKatoh and Standley, 2013.

Graphical analysis of data was performed using GraphPad Prism 6.01 (San Diego, Calif.) and statistical analysis (where indicated) was performed using a paired t-test assuming equal variances. Unless indicated elsewhere graphed data represent the mean±sem.

Example 2. Development of a Multiplex RT-PCR Assay for the Detection of Influenza a, Influenza B, SARS-CoV-2, RSV-A, and RSV-B in Clinical Upper Respiratory Samples

A multiplex assay was developed using the same primers, probes, reagents and methods as in Example 1, with the addition of primers and probes of respiratory syncytial virus subtype A (RSV-A) and respiratory syncytial virus subtype B (RSV-B) (SEQ ID NOs:9-12, 19 and 20) and the substitution of plasmid pFRV19 (SEQ ID NO:29) for plasmid pMK-FluV19 (SEQ ID NO:28), where plasmid pFRV19 includes the addition of RSV-A and RSV-B target sequences (SEQ ID NOs:25 and 26). An annotated map of pFRV19 is shown in FIG. 14.

Results The FRV-19 Multiplex RT-PCR Assay can Detect as Few as 30 Gene Equivalents Per PCR Reaction

Example 1 teaches a FluV19 multiplex RT-PCR assay for detecting Influenza A, Influenza B, and SARS-CoV-2 in clinical samples. The FluV19 laboratory developed assay was tested against the CDC FluSC2 and ThermoFisher TaqMan COVID-19 FluA,FluB Multiplex Assay and demonstrated greater analytical sensitivity and accuracy than either the CDC or ThermoFisher assays (Example 1). Reditus implemented the FluV19 multiplex assay into clinical testing in early 2021 and has been successful in detecting and reporting Influenza and SARS-CoV-2 positive specimens. Due to the recent increase in RSV cases throughout the U.S., we were interested in adding RSV to the panel of viral targets covered by the current FluV19 assay. To this end, primer and probe sets were developed individually against the RNA-Dependent RNA Polymerase (RdRP) of RSV strains A and B. Due to filter constraints of many molecular platforms, both probes developed for detecting RSV-A and RSV-B contain the same 5′ROX reporter and will not be capable of distinguishing between RSV-A and RSV-B during infection. We determined this was not a limitation as there is no significant difference in clinical severity between RSV-A and RSV-B and does not change the course of treatment of infected patients (Laham et al., 2017; Ciarlitto et al., 2019).

Addition of both the RSV-A and RSV-B RdRP gene was also used to redesign the previous pMK-F1UV19 positive control into a new pUC57 backbone herein referred to as pUC57-FRV19. The updated pUC57-FRV19 positive template control contains all gene targets to include: i) Influenza A Matrix 1 protein (M1), ii) Influenza B Non-structural protein (NS1), iii) SARS-CoV-2 Nucleoprotein (N), iv. RSV-A (RdRP), v. RSV-B (RdRP), and iv) p30 subunit of Human RNase P (RP) (FIG. 14).

Therefore, a test was conducted to determine the limit of detection of each target independently (singleplex) and collectively as a part of the combined FRV19 multiplex assay. Briefly, pUC57-FRV19 assay was extracted from transformed E. coli and isolated using the A7510 Wizard® Plus Miniprep DNA Purification System (Promega, Madison, Wis.). Plasmid DNA (pDNA) was quantified using a NanoDrop Onec spectrophotometer (Thermo Fisher Scientific, Waltham, Mass.) and diluted in 10 mM Tris (pH 8.0) to a starting concentration of 1.99×10⁴ viral gene equivalents/W. The pUC57-FRV19 positive template control (PTC) was further diluted in 0.5 log increments to an ending concentration of 2 viral gene equivalents/W. A total of 5 μl of each dilution was tested in triplicate by real-time PCR using reaction volumes and concentrations listed in Table 7. To maintain concentration of primers and probes throughout the PCR reaction, reactions setup to test individual viral targets (singleplex) replaced all other primers and probes with equal volumes of molecular grade water (Table 7).

TABLE 7 FRV19 Multiplex RT-PCR Master Mix 1x 2x 10x 50x 100x Reagent (μl) (μl) (μl) (μl) (μl) InfA Fwd-1 (3.33 μM) 0.5 1.0 5.0 25.0 50.0 InfA Fwd-2 (3.33 μM) 0.5 1.0 5.0 25.0 50.0 InfA Rev-1 (5.0 μM) 0.5 1.0 5.0 25.0 50.0 InfA Rev-2 (1.67 μM) 0.5 1.0 5.0 25.0 50.0 InfA Probe (1.67 μM) 0.5 1.0 5.0 25.0 50.0 InfB Fwd-2 (6.67 μM) 0.5 1.0 5.0 25.0 50.0 InfB Rev-1 (6.67 μM) 0.5 1.0 5.0 25.0 50.0 InfB Probe (1.67 μM) 0.5 1.0 5.0 25.0 50.0 RSV_A Fwd (3.33 μM) 0.5 1.0 5.0 25.0 50.0 RSV_A Rvs (3.33 μM) 0.5 1.0 5.0 25.0 50.0 RSV_A Probe (1.67 μM) 0.5 1.0 5.0 25.0 50.0 RSV_B Fwd (3.33 μM) 0.5 1.0 5.0 25.0 50.0 RSV_B Rvs (3.33 μM) 0.5 1.0 5.0 25.0 50.0 RSV_B Probe (1.67 μM) 0.5 1.0 5.0 25.0 50.0 SARS-CoV-2 Fwd (6.67 μM) 0.5 1.0 5.0 25.0 50.0 SARS-CoV-2 Rev (6.67 μM) 0.5 1.0 5.0 25.0 50.0 SARS-CoV-2 Probe (1.67 μM) 0.5 1.0 5.0 25.0 50.0 RNase P Fwd (9.0 μM) 0.5 1.0 5.0 25.0 50.0 RNase P Rev (9.0 μM) 0.5 1.0 5.0 25.0 50.0 RNase P Probe (3.0 μM) 0.5 1.0 5.0 25.0 50.0 Fast Virus Enzyme (4x) 5.0 10.0 50.0 250.0 500.0 Molecular Grade Water 0.0 0.0 0.0 0.0 0.0 Total Reaction Volume 15.0 30.0 150.0 750.0 1,500.0

Analysis of influenza A by singleplex and multiplex PCR demonstrated an ability to detect the M1 gene as low as 9.95 copies per PCR reaction with <2 Cq difference in detection between singleplex and multiplex assays. When linear regression was applied to assess the efficiency in singleplex and multiplex assays, the coefficient in determination demonstrated a high degree of equivalence between singlplex and multiplex assays (R²=0.9958). Similarly, Influenza B was also detected equally between all dilutions tested with <2 cycles observed in detection between singleplex and multiplex assays and resulted in an R²=0.9974 when regression analysis was applied. Detection of SARS-CoV-2 was also successful at detecting as low as 9.95 copies per PCR reaction but displayed 20-50-times greater ability to detect SARS-CoV-2 at higher N-gene equivalents (99,500-3,150) by singleplex PCR and <4-fold as N-gene copies was reduced from 99.5 N-gene copies per reaction. Regardless, this did not prevent the FRV19 multiplex assay from detecting as low as 9.95 N-gene copies per PCR reaction. Furthermore, regression analysis demonstrated an equivalent correlation between singleplex and multiplex detection of SARS-CoV-2 N-gene with an R²=0.9729. No difference in amplification was observed between singleplex and multiplex detection of RSVA/B across any dilution of pUC57-FRV19 tested with the lower limit of detection being identified at 31.5 RdRP-gene equivalents and a coefficient of determination resulting in an R²=0.9848. Lastly, the RNase P gene was also analyzed as it functions as the internal extraction control present in all human cells in clinical samples. As expected, detection of RNase P (RP) was detected in all 9 dilutions ranging from 99,500 to 9.95 RP-gene equivalents with less than a 5-fold difference in detection with an R²=0.9914 demonstrating equivalence between singleplex and multiplex assays.

The PCR efficiency of the multiplex assay was also calculated based on the standard curve of pUC57-FRV19 with known concentrations of dilutions prepared and tested as part of the limit of detection experiment. Based on the collected data the PCR efficiency of the assay demonstrated an optimized PCR assay as indicated by slopes ≤˜3.2 for all viral target amplification. Thus, the overall PCR efficiency is 92.31±0.063% for influenza A, 95.425±0.085% for influenza B, 96.916±0.122% for SARS-CoV-2, 100.772+0.1% for RSV, and 105.064±0.06% for RNase P.

Collectively, these data demonstrate that the FRV19 multiplex assay is equally as efficient at detecting influenza A, influenza B, SARS-COV-2, RSV, and RNase P as PCR reactions that test targets in individual PCR reactions. While influenza A, influenza B, SARS-CoV-2, and RNase P can be detected as low as 9.95 gene equivalents per PCR reaction, RSV was only able to be consistently detected (i.e. in triplicate) as low as 31.5 gene copies per reaction. Therefore, the lower limit of detection (LOD) of the assay is estimated to be ˜31.5 gene copies per reaction for the FRV19 multiplex assay. Furthermore, based on the mean±sem of triplicate values at the lower limit of each analyte, the cut-off for the assay was set to Cq<37.00 for future experiments. This cutoff was based on detection of all targets as the mean±sem for influenza A, influenza B, SARS-CoV-2, and RNase P approached 37 cycles at the lowest dilution of 31.5 or 9.95 copies per PCR reaction.

Detection of Influenza A, Influenza B, SARS-CoV-2, RSV-A, and RSV-B is not Prohibited in the Presence of Competing Upper Respiratory Pathogens

The limit of detection (LOD) study demonstrated that the FRV19 multiplex assay offered equal detection of influenza A, influenza B, SARS-CoV-2, RSV, and RNase P as detection of each target by individual PCR. However, these data were based exclusively on PCR amplification of targets from the pUC57-FRV19 plasmid. Thus, there was no assessment of amplification following reverse transcription of RNA from either viral targets or the human RNase P gene. Therefore, we sought to determine if the addition of RSV-AB to the FRV19 multiplex assay would reduce the limit of the detection of Influenza A, Influenza B, RSV. or SARS-CoV-2 in clinical samples. To this end, a validation study was conducted using clinicals samples containing competing bacteria and/or viruses which were either: i) virus-negative, ii) single virus-positive, or iii) virus-positive with each combination of viral targets.

A total of 165 SARS-CoV-2-negative clinical samples were selected for use as diluent in preparing validation samples. Samples were collected from anterior, mid-turbinate, and nasopharyngeal swabs in 3 ml of viral transport media (VTM) and were re-tested for the presence for Influenza A, Influenza B, SARS-CoV-2, and RSV by RT-PCR using the FluV19 multiplex assay. All n=165 samples were confirmed negative for SARS-CoV-2. All n=165 samples were detected for RNase P. However, n=3 SARS-CoV-2 negative samples tested positive for influenza A, n=1 sample tested positive for influenza B, and n=1 sample tested positive for RSV. These samples were excluded from testing and/or use as negative specimen diluent. In total, n=160 samples confirmed to be virus-negative were selected for use in preparing clinical validation samples.

To verify specificity of all FRV19 primer and probe targets as well as sensitivity and accuracy of the FR19 multiplex assay, competing bacteria, fungi, and/or viruses were inoculated in each clinical sample. For competing bacteria/fungi, purchased ATCC strains of S. pneumoniae, K pneumoniae, P. aeruginosa, S. epidermidis, C. albicans, S. pyogenes, and a clinical isolate of L. pneumophila serogroup-1 were quantified by culture and optical density. Cultures were pelleted by centrifugation and resuspended in sterile VTM. Bacterial suspensions in VTM were used to inoculate each sample with ≤300 cfu/ml of each respective organism. For competing viruses, purchased ATCC strains of Varicella zoster virus (VZV) and Human Adenovirus C (HAdV-5) were diluted in sterile VTM to achieve ≤300 pfu/ml and used to inoculate each sample.

For preparing specific virus-positive samples, the certificates of analysis provided with purchased ATCC strains of influenza A, influenza B, RSV-A, and RSV-B were used to dilute each specific virus to a concentration of 4,000 pfu/ml in sterile VTM. This represented a 2× stock of each specific virus such that when diluted 1:2 into each specimen (containing competing agents) the final concentration of virus would equal 2,000 pfu/ml. These concentrations are based on a 200 μl extraction and accounting for ˜30% loss of nucleic acid recovery from extraction. Thus, the calculated viral titer at 2,000 pfu/ml was anticipated to be between 2- to 3-times the limit of detection of the FRV19 assay as defined by the following equation:

${{{\frac{2,000{pfu}}{ml} \times \frac{0.2\mspace{14mu}{ml}}{extraction}} = {{\frac{400{pfu}}{extraction} \times \frac{0.27\%\mspace{14mu}{extraction}\mspace{14mu}{loss}}{elution}} = {\frac{108{pfu}}{50\mu\; l\mspace{14mu}{elution}} = {{\frac{20{pfu}}{\mu\; l} \times \frac{5\mu\; l}{{PCR}\mspace{14mu}{Reaction}}} = {\frac{100{pfu}}{{PCR}\mspace{14mu}{reaction}} = {3x}}}}}}’}s\mspace{14mu}{the}\mspace{14mu}{{LOD}.}$

A total of 160 samples were prepared which included n=10 virus-negative samples, and n=10 each of the following virus-positive specimens: i) influenza A, ii) influenza B, iii) SARS-CoV-2, iv) RSV-A, v) RSV-B, vi) influenza A+influenza B, vii) influenza A+SARS-CoV-2, viii) influenza A+RSV-A, ix) influenza A+RSV-B, x) influenza B+SARS-CoV-2, xi) influenza B+RSV-A, xii) influenza B+RSV-B, xiii) SARS-CoV-2+RSV-A, xiv) SARS-CoV-2+RSV-B, and xv) All specific virus targets.

Once prepared, 200 μl of each sample and control was extracted vortexing for 5-10 seconds. The 200 μl non-viral extraction control (NVC) containing 0.1 ng/μl of total Human RNA (Applied Biosystems Cat #4307281) and 200 μl of each sample was transferred into KingFisher 96-well deepwell plates containing 265 μl of lysis buffer and 10 μl of MagMax DNA/RNA binding beads (Applied Biosystems, Cat #A42362). Clinical samples and the NVC were lysed for 1-minute at room temperature followed by addition of 640 μl of 80% Ethanol to each sample. The deepwell plate containing samples were transferred to the KingFisher magnetic particle processor and were extracted using the MVP2_Wash_200_Flex protocol which includes a single wash with 500 μl of Wash Buffer (Materials and Methods), 1,000 μl wash with 80% Ethanol, and 50 μl elution in buffer (Materials and Methods). A total of 5 μl of eluted nucleic acid was amplified using the FRV19 Multiplex RT-PCR Master Mix outlined in Table 7. A PCR positive template control (PTC) was included and consisted of 5 μl of pUC57-FRV19 at a concentration of 2,000 copies/μl for consistent amplification at ˜25 cycles for all targets.

Post amplification analysis was performed using Applied Biosystems Design and Analysis Software v.2.6.0 using a positive cut-off of 37 cycles as defined by the limit of detection study. Analysis of amplification data demonstrated that each independent- and combined-positive specimen were detected within the expected 2- to 3-times LOD ranges. Each of the n=160, clinical samples amplified the Human RNase P gene indicating that each sample contained human epithelial cells collected during swabbing. All of the n=10, virus-negative samples amplified only RNase P and no virus-specific targets. These data demonstrate that neither the >300 cfu/ml competing bacteria/fungi or >300 pfu/ml viruses used in inoculating samples contained any sequences which could either inhibit PCR or generate false-positive amplification results. All single-infected, and co-infected virus-positive samples (Σ=140) were successfully detected for influenza A, influenza B, SARS-COV-2, RSV-A, and RSV-B at the appropriate Cq ranges. Of the n=10, clinical samples containing 20 pfu/μl of each virus, only n=2 samples were undetected for SARS-CoV-2 and would have resulted in false-negative results. While the FRV19 assay was unable to detect these n=2 samples, these samples contained all tested viruses. While it is possible that a single person may be simultaneously infected with all 5 viruses, this scenario is not clinically plausible. Thus, the n=10 specimens containing influenza A, influenza B, SARS-CoV-2, RSV-A, RSV-B, and human cells (RP) were used to the test the limits of the FRV19 assay which succeeded in detecting 58 of the 60 targets (96.7%) across the subset of combined samples.

Clinical analytical statistics were then applied to determine the sensitivity, specificity, precision, and accuracy of the FRV19 assay (Table 8). The FRV19 multiplex RT-PCR assay detected 60/60 (100%) of all influenza A positive samples with no false-negative or false-positive results (Table 8). This resulted in 100% sensitivity, specificity, precision, and accuracy of the FRV19 assay in detecting influenza A in clinical samples (Table 8). Likewise, the FRV19 multiplex assay was 100% sensitive, specific, precise, and accurate in detecting 60/60 influenza B-positive specimens with no false-negative or false-positive results detected (Table 8). Of the n=45, RSV-A- and n=45, RSV-B-positive specimens (1=90), all samples were detected below the cut-off of the assay resulting in 100% for all clinical statistics (Table 8). As mentioned previously, n=2 clinical samples were not detected for SARS-CoV-2 in specimens containing all viruses leading to n=2, SARS-CoV-2 false-negative results obtained by the FRV19 assay. Thus, while the overall specificity and precision of the FRV19 assay to detect SARS-CoV-2 was 100%, the sensitivity and accuracy of detecting SARS-CoV-2 dropped slightly to 96.8% and 98.8%, respectively (Table 8).

TABLE 8 Analytical Statistics Influenza A Values # True Positives (a) 60 # False Positives (c) 0 # True Negatives (d) 100 # False Negatives (b) 0 Sensitivity [a/(a + b)] 100.0% Specificity [d/(c + d)] 100.0% Precision [a/(a + c)] 100.0% Accuracy [(a + d)/(a + b + c + d) 100.0% Analytical Statistics SARS-CoV-2 Values # True Positives (a) 60 # False Positives (c) 0 # True Negatives (d) 100 # False Negatives (b) 2 Sensitivity [a/(a + b)] 96.8% Specificity [d/(c + d)] 100.0% Precision [a/(a + c)] 100.0% Accuracy [(a + d)/(a + b + c + d) 98.8% Analytical Statistics Influenza B Values # True Positives (a) 60 # False Positives (c) 0 # True Negatives (d) 100 # False Negatives (b) 0 Sensitivity [a/(a + b)] 100.0% Specificity [d/(c + d)] 100.0% Precision [a/(a + c)] 100.0% Accuracy [(a + d)/(a + b + c + d) 100.0% Analytical Statistics RSV-A/B Values # True Positives (a) 90 # False Positives (c) 0 # True Negatives (d) 70 # False Negatives (b) 0 Sensitivity [a/(a + b)] 100.0% Specificity [d/(c + d)] 100.0% Precision [a/(a + c)] 100.0% Accuracy [(a + d)/(a + b + c + d) 100.0%

The FRV-19 Multiplex has Low Intra-Assay Variance and Demonstrates Significant Reproducibility Across Time and Temperature

The culmination of data collected thus far demonstrate that the FRV19 assay is a robust and efficient multiplex RT-PCR assay capable of detecting ˜30 viral gene targets per PCR reaction with greater than 98% accuracy in detecting low titers of influenza A, influenza B, SARS-COV-2, and RSV-AB in clinical samples containing high amounts of competing bacteria, fungi, and/or viral pathogens. However, clinical validation samples are tested singly without repeated measures to represent bona fide clinical samples tested in a clinical laboratory. Therefore, we were interested to assess the intra-assay variance of the FRV19 over time and temperatures using already prepared clinical validation samples. Specifically, n=11 validation samples were selected which included a single virus-negative sample and individual specimens positive for: i) influenza A, ii) influenza B, iii) SARS-CoV-2, and iv) RSV-B. Additionally, double virus-positive specimens were also included for: i) influenza A+Influenza B, ii) influenza A+SARS-CoV-2, iii) influenza A+RSV-A, iv) influenza B+SARS-CoV-2, v) Influenza B+RSV-B, and vi) SARS-CoV-2+RSV-B. Each sample was extracted as previously described using 200 μl of sample and amplified by FRV19 multiplex RT-PCR to establish the baseline amplification of each sample on Day 0. Samples were then divided into n=3 aliquots and stored at: 1) 2-8° C., 2) 22-27° C., and 3) 37-40° C. At 24-hour intervals spanning n=5 Days, each sample was extracted in triplicate and amplified using the FRV19 multiplex assay and represents: i) n=60, ii) n=45, iii) n=51, iv) n=57, and v) n=180 independent data points for influenza A, influenza B, SARS-CoV-2, RSV, and RNase P, respectively. The total variance (V_(B)) in the assay was calculated as function of the sum of difference between the Day 0 baseline expected value (V_(E)) and the measured value for the same sample over each 24-hours (V_(T)) divided by the total degrees of freedom per temperature for each analyte. This is represented by the following equation

${V_{B} = \frac{\sum\left\lbrack {{V_{E} - V_{T\; 1}},{V_{E} - V_{T\; 2}},{V_{E} - {V_{T3}\mspace{14mu}\ldots\mspace{14mu} V_{E}} - V_{T25}}} \right\rbrack}{DF}}.$

Collective variance data points were graphed as a function of % Confidence (1/V_(B); y-axis) and temperature (x-axis). Individual variance by sample and temperature was also graphed as function of Cq (y-axis) and Day (x-axis). The metric for determining significance was preestablished for all samples, regardless of temperature, which amplifies the same target ≥3 cycles over Day 0 baseline as this represents a ˜10-fold decrease in detection of that target.

With respect to variance of repeatedly detecting influenza A in clinical samples, no significant difference was observed over the 5 Days, regardless of temperature with the mean±sem of values falling within 98% confidence. These data indicate significant reproducibility of the FRV19 assay to detect influenza A-positive specimens with a high degree of accuracy over time with <1.5 Cq change over Day 0 baseline amplification. Similarly, influenza B demonstrated repeated detection over time and temperature with the mean±sem of variance falling within 98% confidence with <1.5 Cq change, regardless of temperature. Detection of SARS-CoV-2 across time and temperature demonstrated slightly more variance than influenza A or influenza B as the mean±sem of samples were detected with >95% confidence but below the 98% confidence observed for Influenza A and Influenza B. This was also observed individually when variance was tracked for each SARS-CoV-2 positive specimen with Cq ≥2.1 over baseline Day 0 values but which were still <3 Cq, which represents a <10-fold change over baseline. Thus, while slightly higher variance was observed, the repeated ability to detect SARS-CoV-2 is robust with >95% confidence in the system. Detection of RSV demonstrated slightly lower variance in samples stored at 2-8° C. (>98% confidence) than samples stored at 22-27° C. or 37-42° C. (>95% confidence). However, similar to SARS-CoV-2, the repeated capacity to detect RSV-A and RSV-B in clinical samples is significant with <2.1 Cq change over baseline Day 0 amplification. Lastly, detection of RNase P was consistent for datapoints across time and temperature with no depreciable difference in amplification over Day 0 baseline with ≥98 confidence in repeated detection. These data demonstrate the robust reproducibility of the FRV19 multiplex RT-PCR assay in detecting influenza A, influenza B, SARS-CoV-2, and RSV-A/B in clinical samples. Furthermore, these data suggest that samples may be stored at 2-8° C., room temperature (22-27° C.), and are stable when transported in elevated temperatures (37-40° C.) which may occur when cold packs thaw during commercial shipment to laboratories.

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In view of the above, it will be seen that several objectives of the invention are achieved and other advantages attained.

As various changes could be made in the above methods and compositions without departing from the scope of the invention, it is intended that all matter contained in the above description and shown in the accompanying drawings shall be interpreted as illustrative and not in a limiting sense.

All references cited in this specification, including but not limited to patent publications and non-patent literature, and references cited therein, are hereby incorporated by reference. The discussion of the references herein is intended merely to summarize the assertions made by the authors and no admission is made that any reference constitutes prior art. Applicants reserve the right to challenge the accuracy and pertinence of the cited references.

As used herein, in particular embodiments, the terms “about” or “approximately” when preceding a numerical value indicates the value plus or minus a range of 10%. Where a range of values is provided, it is understood that each intervening value, to the tenth of the unit of the lower limit unless the context clearly dictates otherwise, between the upper and lower limit of that range and any other stated or intervening value in that stated range is encompassed within the disclosure. That the upper and lower limits of these smaller ranges can independently be included in the smaller ranges is also encompassed within the disclosure, subject to any specifically excluded limit in the stated range. Where the stated range includes one or both of the limits, ranges excluding either or both of those included limits are also included in the disclosure.

The indefinite articles “a” and “an,” as used herein in the specification and in the embodiments, unless clearly indicated to the contrary, should be understood to mean “at least one.”

The phrase “and/or,” as used herein in the specification and in the embodiments, should be understood to mean “either or both” of the elements so conjoined, i.e., elements that are conjunctively present in some cases and disjunctively present in other cases. Multiple elements listed with “and/or” should be construed in the same fashion, i.e., “one or more” of the elements so conjoined. Other elements can optionally be present other than the elements specifically identified by the “and/or” clause, whether related or unrelated to those elements specifically identified. Thus, as a non-limiting example, a reference to “A and/or B”, when used in conjunction with open-ended language such as “comprising” can refer, in one embodiment, to A only (optionally including elements other than B); in another embodiment, to B only (optionally including elements other than A); in yet another embodiment, to both A and B (optionally including other elements); etc.

As used herein in the specification and in the embodiments, “or” should be understood to have the same meaning as “and/or” as defined above. For example, when separating items in a list, “or” or “and/or” shall be interpreted as being inclusive, i.e., the inclusion of at least one, but also including more than one, of a number or list of elements, and, optionally, additional unlisted items. Only terms clearly indicated to the contrary, such as “only one of” or “exactly one of,” or, when used in the embodiments, “consisting of,” will refer to the inclusion of exactly one element of a number or list of elements. In general, the term “or” as used herein shall only be interpreted as indicating exclusive alternatives (i.e. “one or the other but not both”) when preceded by terms of exclusivity, such as “either,” “one of,” “only one of,” or “exactly one of.” “Consisting essentially of,” when used in the embodiments, shall have its ordinary meaning as used in the field of patent law.

As used herein in the specification and in the embodiments, the phrase “at least one,” in reference to a list of one or more elements, should be understood to mean at least one element selected from any one or more of the elements in the list of elements, but not necessarily including at least one of each and every element specifically listed within the list of elements and not excluding any combinations of elements in the list of elements. This definition also allows that elements can optionally be present other than the elements specifically identified within the list of elements to which the phrase “at least one” refers, whether related or unrelated to those elements specifically identified. Thus, as a non-limiting example, “at least one of A and B” (or, equivalently, “at least one of A or B,” or, equivalently “at least one of A and/or B”) can refer, in one embodiment, to at least one, optionally including more than one, A, with no B present (and optionally including elements other than B); in another embodiment, to at least one, optionally including more than one, B, with no A present (and optionally including elements other than A); in yet another embodiment, to at least one, optionally including more than one, A, and at least one, optionally including more than one, B (and optionally including other elements); etc.

SEQUENCES InfA Fwd-1 SEQ ID NO: 1 CAAGACCAATCYTGTCACCTCTGAC InfA Fwd-2 SEQ ID NO: 2 CAAGACCAATYCTGTCACCTYTGAC InfA Rev-1  SEQ ID NO: 3 GCATTYTGGACAAAVCGTCTACG InfA Rev-2 SEQ ID NO: 4 GCATTTTGGATAAAGCGTCTACG InfBFwd SEQ ID NO: 5 TCCTCAAYTCACTCTTCGAGCG InfBRev SEQ ID NO: 6 CGGTGCTCTTGACCAAATTGG SARSCoV2Fwd SEQ ID NO: 7 CTGCAGATTTGGATGATTTCTCC SARSCoV2Rvs SEQ ID NO: 8 CCTTGTGTGGTCTGCATGAGTTTAG RSV-A Fwd SEQ ID NO: 9 ACCAACTTAATTAGTAGACAAAATCCA RSV-A Rvs SEQ ID NO: 10 TCTGACGAGGTCATACTCTTGT RSV-B Fwd SEQ ID NO: 11 GCATAAGTTTTGGTCTTAGCTTGA RSV-B Rvs SEQ ID NO: 12 AAATGTATCTCATTCAGCTTCGGT RNP Fwd SEQ ID NO: 13 AGATTTGGACCTGCGAGCG RNP Rvs SEQ ID NO: 14 GAGCGGCTGTCTCCACAAGT InfAProbe SEQ ID NO: 15 [Cy5]TGCAGTCCTCGCTCACTGGGCACG[BHQ2a-Q] InfBProbe SEQ ID NO: 16 [HEX]CCAATTCGAGCAGCTGAAACTGCGGTG[BHQ1a-Q] SARSCoV2Probe SEQ ID NO: 17 [6FAM]ATTGCAACAATCCATGAGCAGTGCTGACTC[BHQ1a-Q] RNP Probe SEQ ID NO: 18 [TAMRA]TTCTGACCTGAAGGCTCTGCGCG[BHQ2a-Q] RSV-A Probe SEQ ID NO: 19 [ROX]AGAAGAACCTACTTACTTTCAGTCA[BHQ2a-Q] RSV-B Probe SEQ ID NO: 20 [ROX]TGGAACAATTCACAAACATATGTCCT[BHQ2a-Q] Influenza A Conserved Matrix Protein 2 (M2) Target Sequence (168 bp) SEQ ID NO: 21 TGTCCAGAGCTCCTCGAGATGGAATGGCTAAAGACAAGACCAATCTTGTC ACCTCTGACTAAGGGAATTTTAGGATTTGTGTTCACGCTCACCGTGCCCA GTGAGCGAGGACTGCAGCGTAGACGCTTTGTCCAAAATGCCCTAAATGGG AATGGGGACCCGTCTAGA Influenza B Conserved Non-Structural Protein 1 (NS1) Target Sequence (156 bp) SEQ ID NO: 22 AACAACATGGCCATCGGATCCTCAATTCACTCTTCGAGCGTCTTAATGAA GGACATTCAAAGCCAATTCGAGCAGCTGAAACTGCGGTGGGAGTCTTATC CCAATTTGGTCAAGAGCACCGACTATCACCAGAAGAGGGAGACAAAACAG ACTAGT SARS-CoV-2 ORF lab Target Sequence(150 bp) SEQ ID NO: 23 CAAACTGTGACTCTTCTTCCTGCTGCAGATTTGGATGATTTCTCCAAACA ATTGCAACAATCCATGAGCAGTGCTGACTCAACTCAGGCCTAAACTCATG CAGACCACACAAGGCAGATGGGCTATATAAACGTTTTCGCTTTTCATATG Human RNaseP Target Sequence (129 bp) SEQ ID NO: 24 CCGTTTACGATGGCGGTGTTTGCAGATTTGGACCTGCGAGCGGGTTCTGA CCTGAAGGCTCTGCGCGGACTTGTGGAGACAGCCGCTCACCTTGGCTATT CAGTTGTTGCTATCAATCCATGGGGTACC RSV-A Target Sequence SEQ ID NO: 25 TTACATATTCAATGGTCCTTATCTCAAAAATGATTATACCAACTTAATTA GTAGACAAAATCCATTAATAGAACACATAAATCTAAAGAAACTAAATATA ACACAGTCCTTAATATCTAAGTATCAT RSV-B Target Sequence SEQ ID NO: 26 GACATTGTGTTTCAAAATTGCATAAGTTTTGGTCTTAGCTTGATGTCAGT TGTGGAACAATTCACAAACATATGTCCTAATAGAATTATTCTCATACCGA AGCTGAATGAGATACATTTGATGAAAC Kanamycin Resistance Sequence SEQ ID NO: 27 ATGATTGAACAGGATGGCCTGCATGCGGGTAGCCCGGCAGCGTGGGTGGA ACGTCTGTTTGGCTATGATTGGGCGCAGCAGACCATTGGCTGCTCTGATG CGGCGGTGTTTCGTCTGAGCGCGCAGGGTCGTCCGGTGCTGTTTGTGAAA ACCGATCTGAGCGGTGCGCTGAACGAGCTGCAGGATGAAGCGGCGCGTCT GAGCTGGCTGGCCACCACCGGTGTTCCGTGTGCGGCGGTGCTGGATGTGG TGACCGAAGCGGGCCGTGATTGGCTGCTGCTGGGCGAAGTGCCGGGTCAG GATCTGCTGTCTAGCCATCTGGCGCCGGCAGAAAAAGTGAGCATTATGGC GGATGCCATGCGTCGTCTGCATACCCTGGACCCGGCGACCTGTCCGTTTG ATCATCAGGCGAAACATCGTATTGAACGTGCGCGTACCCGTATGGAAGCG GGCCTGGTGGATCAGGATGATCTGGATGAAGAACATCAGGGCCTGGCACC GGCAGAGCTGTTTGCGCGTCTGAAAGCGAGCATGCCGGATGGCGAAGATC TGGTGGTGACCCATGGTGATGCGTGCCTGCCGAACATTATGGTGGAAAAT GGCCGTTTTAGCGGCTTTATTGATTGCGGCCGTCTGGGCGTGGCGGATCG TTATCAGGATATTGCGCTGGCCACCCGTGATATTGCGGAAGAACTGGGCG GCGAATGGGCGGATCGTTTTCTGGTGCTGTATGGCATTGCGGCACCGGAT AGCCAGCGTATTGCGTTTTATCGTCTGCTGGATGAATTTTTCTAATAA pMK-FluV19 SEQ ID NO: 28 CTAAATTGTAAGCGTTAATATTTTGTTAAAATTCGCGTTAAATTTTTGTT AAATCAGCTCATTTTTTAACCAATAGGCCGAAATCGGCAAAATCCCTTAT AAATCAAAAGAATAGACCGAGATAGGGTTGAGTGGCCGCTACAGGGCGCT CCCATTCGCCATTCAGGCTGCGCAACTGTTGGGAAGGGCGTTTCGGTGCG GGCCTCTTCGCTATTACGCCAGCTGGCGAAAGGGGGATGTGCTGCAAGGC GATTAAGTTGGGTAACGCCAGGGTTTTCCCAGTCACGACGTTGTAAAACG ACGGCCAGTGAGCGCGACGTAATACGACTCACTATAGGGCGAATTGAAGG AAGGCCGTCAAGGCCACGTGTCTTGTCCAGAGCTCCTCGAGATGGAATGG CTAAAGACAAGACCAATCTTGTCACCTCTGACTAAGGGAATTTTAGGATT TGTGTTCACGCTCACCGTGCCCAGTGAGCGAGGACTGCAGCGTAGACGCT TTGTCCAAAATGCCCTAAATGGGAATGGGGACCCGTCTAGAAACAACATG GCCATCGGATCCTCAATTCACTCTTCGAGCGTCTTAATGAAGGACATTCA AAGCCAATTCGAGCAGCTGAAACTGCGGTGGGAGTCTTATCCCAATTTGG TCAAGAGCACCGACTATCACCAGAAGAGGGAGACAAAACAGACTAGTCAA ACTGTGACTCTTCTTCCTGCTGCAGATTTGGATGATTTCTCCAAACAATT GCAACAATCCATGAGCAGTGCTGACTCAACTCAGGCCTAAACTCATGCAG ACCACACAAGGCAGATGGGCTATATAAACGTTTTCGCTTTTCATATGCCG TTTACGATGGCGGTGTTTGCAGATTTGGACCTGCGAGCGGGTTCTGACCT GAAGGCTCTGCGCGGACTTGTGGAGACAGCCGCTCACCTTGGCTATTCAG TTGTTGCTATCAATCCATGGGGTACCTGGAGCACAAGACTGGCCTCATGG GCCTTCCTTTCACTGCCCGCTTTCCAGTCGGGAAACCTGTCGTGCCAGCT GCATTAACATGGTCATAGCTGTTTCCTTGCGTATTGGGCGCTCTCCGCTT CCTCGCTCACTGACTCGCTGCGCTCGGTCGTTCGGGTAAAGCCTGGGGTG CCTAATGAGCAAAAGGCCAGCAAAAGGCCAGGAACCGTAAAAAGGCCGCG TTGCTGGCGTTTTTCCATAGGCTCCGCCCCCCTGACGAGCATCACAAAAA TCGACGCTCAAGTCAGAGGTGGCGAAACCCGACAGGACTATAAAGATACC AGGCGTTTCCCCCTGGAAGCTCCCTCGTGCGCTCTCCTGTTCCGACCCTG CCGCTTACCGGATACCTGTCCGCCTTTCTCCCTTCGGGAAGCGTGGCGCT TTCTCATAGCTCACGCTGTAGGTATCTCAGTTCGGTGTAGGTCGTTCGCT CCAAGCTGGGCTGTGTGCACGAACCCCCCGTTCAGCCCGACCGCTGCGCC TTATCCGGTAACTATCGTCTTGAGTCCAACCCGGTAAGACACGACTTATC GCCACTGGCAGCAGCCACTGGTAACAGGATTAGCAGAGCGAGGTATGTAG GCGGTGCTACAGAGTTCTTGAAGTGGTGGCCTAACTACGGCTACACTAGA AGAACAGTATTTGGTATCTGCGCTCTGCTGAAGCCAGTTACCTTCGGAAA AAGAGTTGGTAGCTCTTGATCCGGCAAACAAACCACCGCTGGTAGCGGTG GTTTTTTTGTTTGCAAGCAGCAGATTACGCGCAGAAAAAAAGGATCTCAA GAAGATCCTTTGATCTTTTCTACGGGGTCTGACGCTCAGTGGAACGAAAA CTCACGTTAAGGGATTTTGGTCATGAGATTATCAAAAAGGATCTTCACCT AGATCCTTTTAAATTAAAAATGAAGTTTTAAATCAATCTAAAGTATATAT GAGTAAACTTGGTCTGACAGTTATTAGAAAAATTCATCCAGCAGACGATA AAACGCAATACGCTGGCTATCCGGTGCCGCAATGCCATACAGCACCAGAA AACGATCCGCCCATTCGCCGCCCAGTTCTTCCGCAATATCACGGGTGGCC AGCGCAATATCCTGATAACGATCCGCCACGCCCAGACGGCCGCAATCAAT AAAGCCGCTAAAACGGCCATTTTCCACCATAATGTTCGGCAGGCACGCAT CACCATGGGTCACCACCAGATCTTCGCCATCCGGCATGCTCGCTTTCAGA CGCGCAAACAGCTCTGCCGGTGCCAGGCCCTGATGTTCTTCATCCAGATC ATCCTGATCCACCAGGCCCGCTTCCATACGGGTACGCGCACGTTCAATAC GATGTTTCGCCTGATGATCAAACGGACAGGTCGCCGGGTCCAGGGTATGC AGACGACGCATGGCATCCGCCATAATGCTCACTTTTTCTGCCGGCGCCAG ATGGCTAGACAGCAGATCCTGACCCGGCACTTCGCCCAGCAGCAGCCAAT CACGGCCCGCTTCGGTCACCACATCCAGCACCGCCGCACACGGAACACCG GTGGTGGCCAGCCAGCTCAGACGCGCCGCTTCATCCTGCAGCTCGTTCAG CGCACCGCTCAGATCGGTTTTCACAAACAGCACCGGACGACCCTGCGCGC TCAGACGAAACACCGCCGCATCAGAGCAGCCAATGGTCTGCTGCGCCCAA TCATAGCCAAACAGACGTTCCACCCACGCTGCCGGGCTACCCGCATGCAG GCCATCCTGTTCAATCATACTCTTCCTTTTTCAATATTATTGAAGCATTT ATCAGGGTTATTGTCTCATGAGCGGATACATATTTGAATGTATTTAGAAA AATAAACAAATAGGGGTTCCGCGCACATTTCCCCGAAAAGTGCCAC pFRV19 SEQ ID NO: 29 TCGCGCGTTTCGGTGATGACGGTGAAAACCTCTGACACATGCAGCTCCCG GAGACGGTCACAGCTTGTCTGTAAGCGGATGCCGGGAGCAGACAAGCCCG TCAGGGCGCGTCAGCGGGTGTTGGCGGGTGTCGGGGCTGGCTTAACTATG CGGCATCAGAGCAGATTGTACTGAGAGTGCACCATATGCGGTGTGAAATA CCGCACAGATGCGTAAGGAGAAAATACCGCATCAGGCGCCATTCGCCATT CAGGCTGCGCAACTGTTGGGAAGGGCGATCGGTGCGGGCCTCTTCGCTAT TACGCCAGCTGGCGAAAGGGGGATGTGCTGCAAGGCGATTAAGTTGGGTA ACGCCAGGGTTTTCCCAGTCACGACGTTGTAAAACGACGGCCAGAGAATT CGAGCTCGGTACCTCGCGAATACATCTAGATCTCGAGATTCAGGTTACAT ATTCAATGGTCCTTATCTCAAAAATGATTATACCAACTTAATTAGTAGAC AAAATCCATTAATAGAACACATAAATCTAAAGAAACTAAATATAACACAG TCCTTAATATCTAAGTATCATAAAGGTGAAATAAAAATAGAAGAACCTAC TTACTTTCAGTCATTACTTATGACATACAAGAGTATGACCTCGTCAGAAC AGACTACTACTACTAATTTACTTAAAAAGATAATAAGAAGAGCTCGACAT TGTGTTTCAAAATTGCATAAGTTTTGGTCTTAGCTTGATGTCAGTTGTGG AACAATTCACAAACATATGTCCTAATAGAATTATTCTCATACCGAAGCTG AATGAGATACATTTGATGAAACCTCCTATATTTACAGGAGATGTTGATAT CATCAAGTTGAAGCAAGTGATACAAAAACAGGAATGGCTAAAGACAAGAC CAATCTTGTCACCTCTGACTAAGGGAATTTTAGGATTTGTGTTCACGCTC ACCGTGCCCAGTGAGCGAGGACTGCAGCGTAGACGCTTTGTCCAAAATGC CCTAAATGGGAATGGGGACCCGTCTAGAAACAACATGGCCATCGGATCCT CAATTCACTCTTCGAGCGTCTTAATGAAGGACATTCAAAGCCAATTCGAG CAGCTGAAACTGCGGTGGGAGTCTTATCCCAATTTGGTCAAGAGCACCGA CTATCACCAGAAGAGGGAGACAAAACAGACTAGTCAAACTGTGACTCTTC TTCCTGCTGCAGATTTGGATGATTTCTCCAAACAATTGCAACAATCCATG AGCAGTGCTGACTCAACTCAGGCCTAAACTCATGCAGACCACACAAGGCA GATGGGCTATATAAACGTTTTCGCTTTTCATATGCCGTTTACGATGGCGG TGTTTGCAGATTTGGACCTGCGAGCGGGTTCTGACCTGAAGGCTCTGCGC GGACTTGTGGAGACAGCCGCTCACCTTGGCTATTCAGTTGTTGCTATCAA TCCATGGATCGGATCCCGGGCCCGTCGACTGCAGAGGCCTGCATGCAAGC TTGGTGTAATCATGGTCATAGCTGTTTCCTGTGTGAAATTGTTATCCGCT CACAATTCCACACAACATACGAGCCGGAAGCATAAAGTGTAAAGCCTGGG GTGCCTAATGAGTGAGCTAACTCACATTAATTGCGTTGCGCTCACTGCCC GCTTTCCAGTCGGGAAACCTGTCGTGCCAGCTGCATTAATGAATCGGCCA ACGCGCGGGGAGAGGCGGTTTGCGTATTGGGCGCTCTTCCGCTTCCTCGC TCACTGACTCGCTGCGCTCGGTCGTTCGGCTGCGGCGAGCGGTATCAGCT CACTCAAAGGCGGTAATACGGTTATCCACAGAATCAGGGGATAACGCAGG AAAGAACATGTGAGCAAAAGGCCAGCAAAAGGCCAGGAACCGTAAAAAGG CCGCGTTGCTGGCGTTTTTCCATAGGCTCCGCCCCCCTGACGAGCATCAC AAAAATCGACGCTCAAGTCAGAGGTGGCGAAACCCGACAGGACTATAAAG ATACCAGGCGTTTCCCCCTGGAAGCTCCCTCGTGCGCTCTCCTGTTCCGA CCCTGCCGCTTACCGGATACCTGTCCGCCTTTCTCCCTTCGGGAAGCGTG GCGCTTTCTCATAGCTCACGCTGTAGGTATCTCAGTTCGGTGTAGGTCGT TCGCTCCAAGCTGGGCTGTGTGCACGAACCCCCCGTTCAGCCCGACCGCT GCGCCTTATCCGGTAACTATCGTCTTGAGTCCAACCCGGTAAGACACGAC TTATCGCCACTGGCAGCAGCCACTGGTAACAGGATTAGCAGAGCGAGGTA TGTAGGCGGTGCTACAGAGTTCTTGAAGTGGTGGCCTAACTACGGCTACA CTAGAAGAACAGTATTTGGTATCTGCGCTCTGCTGAAGCCAGTTACCTTC GGAAAAAGAGTTGGTAGCTCTTGATCCGGCAAACAAACCACCGCTGGTAG CGGTGGTTTTTTTGTTTGCAAGCAGCAGATTACGCGCAGAAAAAAAGGAT CTCAAGAAGATCCTTTGATCTTTTCTACGGGGTCTGACGCTCAGTGGAAC GAAAACTCACGTTAAGGGATTTTGGTCATGAGATTATCAAAAAGGATCTT CACCTAGATCCTTTTAAATTAAAAATGAAGTTTTAAATCAAGCCCAATCT GAATAATGTTACAACCAATTAACCAATTCTGATTAGAAAAACTCATCGAG CATCAAATGAAACTGCAATTTATTCATATCAGGATTATCAATACCATATT TTTGAAAAAGCCGTTTCTGTAATGAAGGAGAAAACTCACCGAGGCAGTTC CATAGGATGGCAAGATCCTGGTATCGGTCTGCGATTCCGACTCGTCCAAC ATCAATACAACCTATTAATTTCCCCTCGTCAAAAATAAGGTTATCAAGTG AGAAATCACCATGAGTGACGACTGAATCCGGTGAGAATGGCAAAAGTTTA TGCATTTCTTTCCAGACTTGTTCAACAGGCCAGCCATTACGCTCGTCATC AAAATCACTCGCATCAACCAAACCGTTATTCATTCGTGATTGCGCCTGAG CGAGACGAAATACGCGATCGCTGTTAAAAGGACAATTACAAACAGGAATC GAATGCAACCGGCGCAGGAACACTGCCAGCGCATCAACAATATTTTCACC TGAATCAGGATATTCTTCTAATACCTGGAATGCTGTTTTTCCGGGGATCG CAGTGGTGAGTAACCATGCATCATCAGGAGTACGGATAAAATGCTTGATG GTCGGAAGAGGCATAAATTCCGTCAGCCAGTTTAGTCTGACCATCTCATC TGTAACATCATTGGCAACGCTACCTTTGCCATGTTTCAGAAACAACTCTG GCGCATCGGGCTTCCCATACAAGCGATAGATTGTCGCACCTGATTGCCCG ACATTATCGCGAGCCCATTTATACCCATATAAATCAGCATCCATGTTGGA ATTTAATCGCGGCCTCGACGTTTCCCGTTGAATATGGCTCATAACACCCC TTGTATTACTGTTTATGTAAGCAGACAGTTTTATTGTTCATGATGATATA TTTTTATCTTGTGCAATGTAACATCAGAGATTTTGAGACACGGGCCAGAG CTGCA 

What is claimed is:
 1. A GRD buffer system for extracting nucleic acid, the GRD buffer system comprising: a GRD lysis buffer (GRD-LB), wherein the GRD-LB comprises a first buffer and a first chaotropic agent; a GRD wash buffer (GRD-WB), wherein the GRD-WB comprises a second buffer, a second chaotropic agent, and an alcohol; a GRD elution buffer (GRD-EB), wherein the GRD-EB comprises a third buffer; and the GRD buffer system is free of proteinase K.
 2. The GRD buffer system of claim 1, wherein: the GRD-LB further comprises a first chelating agent, a first detergent, a first denaturant, and a dye; the GRD-WB further comprises a second chelating agent; and the GRD-EB further comprises a third chelating agent.
 3. The GRD buffer system of claim 1 or 2, wherein: the first buffer is Bis-Tris Propane, TES, HEPES, DIPSO, MOBS, TAPSO, Tris, Trizma, HEPPSO, POPSO, TEA, EPPS, Tricine, Gly-Gly, Bicine, HEPBS, TAPS, and AMPD; the first chelating agent is EDTA, EGTA, HEDTA, NTA, and TEA; the first detergent is Triton X-100, TWEEN-20, NP-40, and Brij-35; the first denaturant is formamide, guanidine, sodium salicylate, dimethyl sulfoxide (DMSO), propylene glycol, and urea; the dye is bromophenol blue, xylene cyanol, and orange G; the first chaotropic agent is guanidinium thiocyanate, guanidine, urea, and thiourea; the second buffer is Bis-Tris Propane, TES, HEPES, DIPSO, MOBS, TAPSO, Tris, Trizma, HEPPSO, POPSO, TEA, EPPS, Tricine, Gly-Gly, Bicine, HEPBS, TAPS, and AMPD; the second chelating agent is EDTA, EGTA, HEDTA, NTA, and TEA; the second chaotropic agent is guanidinium thiocyanate, guanidine, urea, and thiourea; the alcohol is methanol, ethanol, and isopropanol; the third buffer is Bis-Tris Propane, TES, HEPES, DIPSO, MOBS, TAPSO, Tris, Trizma, HEPPSO, POPSO, TEA, EPPS, Tricine, Gly-Gly, Bicine, HEPBS, TAPS, and AMPD; and the third chelating agent is EDTA, EGTA, HEDTA, NTA, and TEA.
 4. The GRD buffer system of claim 3, wherein: the first buffer is Tris; the first chelating agent is EDTA; the first detergent is Triton X-100; the first denaturant is urea; the dye is bromophenol blue; the first chaotropic agent is guanidinium thiocyanate; the second buffer is Tris; the second chelating agent is EDTA; the second chaotropic agent is guanidinium thiocyanate; the alcohol is ethanol; the third buffer is Tris; and the third chelating agent is EDTA.
 5. The GRD buffer system of claim 3 or 4, wherein: the first buffer is Tris (pH 8.0, Cf=50 mM); the first chelating agent is EDTA (pH 8.0, Cf=25 mM); the first detergent is Triton X-100 (3% v/v); the first denaturant is urea (Cf=10 mM); the dye is bromophenol blue (Cf=0.01% v/v); the first chaotropic agent is guanidinium thiocyanate (Cf=4 M); the second buffer is Tris (pH 8.0, Cf=10 mM); the second chelating agent is EDTA (pH 8.0, 7.5 mM); the second chaotropic agent is guanidinium thiocyanate (Cf=1.82 M); the alcohol is ethanol (Cf=70% v/v); the third buffer is Tris (pH 8.0, Cf=100 mM); and the third chelating agent is EDTA (pH 8.0, 10 mM).
 6. A method of extracting nucleic acid with the GRD buffer system of claim 1, the method comprising: providing a sample; and extracting nucleic acid with the GRD buffer system.
 7. The method of claim 6, wherein the sample is from a nasal swab, a nasopharyngeal swab, or a throat swab.
 8. The method of claim 6 or 7, wherein the sample contains a respiratory virus.
 9. The method of claim 8, wherein the respiratory virus is influenza A, influenza B, SARS-CoV-2, respiratory syncytial virus subtype A, respiratory syncytial virus subtype B, or any combination thereof. 